A Compartmentalized Mathematical Model of the β1-Adrenergic Signaling System in Mouse Ventricular Myocytes

Vladimir E. Bondarenko

doi:10.1371/journal.pone.0089113

Abstract

The β₁-adrenergic signaling system plays an important role in the functioning of cardiac cells. Experimental data shows that the activation of this system produces inotropy, lusitropy, and chronotropy in the heart, such as increased magnitude and relaxation rates of [Ca²⁺]_i transients and contraction force, and increased heart rhythm. However, excessive stimulation of β₁-adrenergic receptors leads to heart dysfunction and heart failure. In this paper, a comprehensive, experimentally based mathematical model of the β₁-adrenergic signaling system for mouse ventricular myocytes is developed, which includes major subcellular functional compartments (caveolae, extracaveolae, and cytosol). The model describes biochemical reactions that occur during stimulation of β₁-adrenoceptors, changes in ionic currents, and modifications of Ca²⁺ handling system. Simulations describe the dynamics of major signaling molecules, such as cyclic AMP and protein kinase A, in different subcellular compartments; the effects of inhibition of phosphodiesterases on cAMP production; kinetics and magnitudes of phosphorylation of ion channels, transporters, and Ca²⁺ handling proteins; modifications of action potential shape and duration; magnitudes and relaxation rates of [Ca²⁺]_i transients; changes in intracellular and transmembrane Ca²⁺ fluxes; and [Na⁺]_i fluxes and dynamics. The model elucidates complex interactions of ionic currents upon activation of β₁-adrenoceptors at different stimulation frequencies, which ultimately lead to a relatively modest increase in action potential duration and significant increase in [Ca²⁺]_i transients. In particular, the model includes two subpopulations of the L-type Ca²⁺ channels, in caveolae and extracaveolae compartments, and their effects on the action potential and [Ca²⁺]_i transients are investigated. The presented model can be used by researchers for the interpretation of experimental data and for the developments of mathematical models for other species or for pathological conditions.

Citation: Bondarenko VE (2014) A Compartmentalized Mathematical Model of the β₁-Adrenergic Signaling System in Mouse Ventricular Myocytes. PLoS ONE 9(2): e89113. https://doi.org/10.1371/journal.pone.0089113

Editor: Xun Ai, Loyola University Chicago, United States of America

Received: September 29, 2013; Accepted: January 14, 2014; Published: February 21, 2014

Copyright: © 2014 Vladimir E. Bondarenko. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Funding: This work was supported by the American Heart Association (http://www.heart.org/HEARTORG/) (10GRNT4720012), Georgia State University (http://www.gsu.edu) Seed Grant from Brain and Behavior Program, and Research Initiation Grant to V. E. Bondarenko. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: Vladimir Bondarenko is an Academic Editor of PLOS ONE. This does not alter his adherence to all the PLOS ONE policies on sharing data and materials.

Introduction

Cardiac cells belong to a wide class of excitable cells which include electrical activity, Ca²⁺ dynamics, and protein signaling networks. While early experimental studies of cardiac cells are predominantly devoted to their electrical activity, and later to Ca²⁺ dynamics, more recent studies involve investigations of protein signaling systems, which modulate both action potentials and intracellular Ca²⁺ transients [1], [2]. On the tissue and whole heart levels, the activation of such signaling systems either promotes or suppresses pro-arrhythmic behavior. In addition, in diseased hearts, protein signaling networks become modified and do not properly regulate the electrical activity or Ca²⁺ handling system [3]. As a result, the studies of major signaling protein networks in cardiac cells identified new potential therapeutic targets for treatment of heart diseases; some of the targets include signaling proteins involved in β₁-adrenergic signaling system [4], [5], [6], [7].

Mathematical modeling of protein signaling networks is a supplementary tool for understanding their functions in the heart. Recently, particular attention has been paid to the development of comprehensive models for β₁-adrenergic system in ventricular myocytes of different species [8], [9], [10], [11], [12]. The first model developed by Saucerman et al. [10] for rat ventricular myocytes set high standards for simulation of the β₁-adrenergic signaling system. The model included biochemical and electrophysiological parts with two major protein kinase A targets, phospholamban and the L-type Ca²⁺ channel, and consisted of one cytosolic compartment (single-compartment model). Later, a similar model was developed for rabbit ventricular myocytes and included several new PKA targets: ryanodine receptors, troponin I, and slow delayed rectifier K⁺ current, I_Ks [11]. The model was further extended to simulate the effects of the β₁-adrenergic signaling system in mouse ventricular myocytes, predominantly on Ca²⁺ dynamics [12]. Finally, a model of β₁-adrenergic signaling system in guinea pig ventricular myocytes [9] was developed based on the model of Saucerman et al. [10], which is devoted to the analysis of the changes in action potential, intracellular [Ca²⁺]_i transients, and ionic fluxes upon stimulation of β₁-adrenoceptors with agonist isoproterenol.

Simultaneously, multi-compartmental models of protein signaling networks, including the β₁-adrenergic signaling system, were developed [8], [13], [14]. The compartmentalized models of Iancu et al. [13], [14] included only the biochemical part of β₁-adrenergic and M₂-muscarinic signaling systems and described the dynamics of cAMP and PKA in different subcellular compartments (caveolae, extracaveolae, and cytosol). The only compartmentalized model of cardiac protein signaling network, which includes both biochemical and electrophysiological parts, β₁- and β₂-adrenergic and CaMKII-mediated signaling systems, was developed recently for canine ventricular myocytes by Heijman et al. [8]. The model was extensively verified by experimental data and reproduced major features of stimulation of the three signaling systems.

Compartmentalization of the signaling systems in cardiac cells is an important property. This property allows for regulation of multiple cellular functions, such as electrical activity, Ca²⁺ dynamics, and cellular contraction (for examples see reviews [1], [15], [16], [17], [18]). The experimental data demonstrates differential localization of the components of the Ca²⁺-mediated, α- and β-adrenergic signaling systems [19], [20], [21], [22]. In cardiac myocytes, β₁-adrenergic receptors are mostly localized in membrane compartments that lack caveolin-3, while β₂-adrenergic receptors are mostly found in caveolin-3-rich domains [20]. Investigations of the physiological role of the β-receptors have shown their differing effects in the development of disease states: excessive activation of β₁-adrenergic signaling led to cardiac hypertrophy and heart failure [23], while moderately increased stimulation of β₂-adrenergic signaling was cardioprotective [24]. In addition, β₁- and β₂-adrenergic receptors modulate differently cardiac ionic currents and contraction proteins, which are also localized in different cellular compartments [15], [16]. In the β₁-adrenergic signaling system alone, which is the major topic of this paper, multiple signaling molecules are also distributed among the major cellular compartments related to caveolin-3, non-caveolae cellular membrane, or cytosol, and these molecules are differentially modulated upon activation of β₁-receptors. In particular, the recent discovery of the two subpopulations of the L-type Ca²⁺ channels, the major players in cardiac excitation-contraction coupling, which are localized in caveolin-3-rich and non-caveolae compartments and play different physiological roles, requires more comprehensive, compartmentalized models of cardiac cells [22].

In this paper, we developed a new compartmentalized model for the β₁-adrenergic signaling system in mouse ventricular myocytes. The model is based on our previously published models for action potential and Ca²⁺ dynamics in mouse ventricular myocytes [25], [26]. The new model includes both biochemical and electrophysiological parts, as well as compartmentalization of the β₁-adrenergic signaling system, which includes three major compartments: caveolae, extracaveolae, and cytosol. Both biochemical and electrophysiological parts are verified by extensive experimental data, primarily obtained from the rodent cardiac cells. Activation of the major proteins in the signaling system, such as adenylyl cyclases and phosphodiesterases, is compared directly to the data from the mouse ventricular myocytes in absolute magnitudes. The model successfully reproduced existing experimental data on cAMP dynamics, activation of adenylyl cyclases and phosphodiesterases, protein kinase A and phosphorylation of its targets, and the effects of phosphodiesterases inhibition on cAMP transients. Simulations also reproduced data obtained from voltage-clamp protocols for major repolarization currents of mouse ventricular myocytes. The model is able to simulate action potential shape and duration upon stimulation of β₁-adrenergic receptors (β₁-ARs). The model elucidated the mechanism of relatively moderate AP prolongation, significant increase in intracellular [Ca²⁺]_i transients, modification of the intracellular and transmembrane Ca²⁺ fluxes, and [Na⁺]_i fluxes and dynamics. The model includes two pools of the L-type Ca²⁺ channels, one in the caveolae and the other in the extracaveolae compartments. The simulations demonstrated their different modulations upon stimulation of β₁-ARs and their different effects on the action potentials and [Ca²⁺]_i transients. The model simulated frequency dependences of [Ca²⁺]_i transient decays for control conditions and after stimulation of β₁-ARs, and made testable predictions for the frequency dependences of [Ca²⁺]_i transient amplitudes, AP amplitudes and durations. The simulation results are compared to the results obtained from other models of β₁-adrenergic signaling system in other species, and the model limitations are discussed.

Methods

A mathematical model for the β₁-adrenergic signaling system in mouse ventricular myocytes is a natural extension of the previously published model for action potential and Ca²⁺ dynamics in mouse ventricular myocytes [25], with model improvements from [26] (Fig. 1). We incorporated a β₁-adrenergic signaling pathway in our model of electrical activity and Ca²⁺ handling with modifications [25], [26] (see Appendix S1).

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Figure 1. Schematic representation of the β₁-adrenergic signaling system in mouse ventricular myocytes.

Transmembrane currents are the fast Na⁺ current (I_Na), the two components of the L-type Ca²⁺ current in caveolae and extracaveolae compartments (I_CaL,cav and I_CaL,ecav, respectively), the sarcolemmal Ca²⁺ pump (I_p(Ca)), the Na⁺/Ca²⁺ exchanger (I_NaCa), the rapidly recovering transient outward K⁺ current (I_Kto,f), the rapid delayed rectifier K⁺ current (I_Kr), the ultrarapidly activating delayed rectifier K⁺ current (I_Kur), the noninactivating steady-state voltage activated K⁺ current (I_Kss), the time-independent K⁺ current (I_K1), the Na⁺/K⁺ pump (I_NaK, is regulated by phospholemman, PLM), the Ca²⁺ and Na⁺ background currents (I_Cab and I_Nab). The Ca²⁺ fluxes are uptake of Ca²⁺ from the cytosol to the network sarcoplasmic reticulum (NSR) (J_up) by the SERCA pump and Ca²⁺ release from the junctional sarcoplasmic reticulum (JSR) (J_rel) through the ryanodine receptors (RyRs). There are three intracellular compartments in the β₁-adrenergic signaling system: caveolae, extracaveolae, and cytosol. The subspace volume (V_ss) is located in the extracaveolae domain. Components of the β₁-adrenergic signaling system are the β₁-adrenergic receptors (β1-AR), the α-subunit of stimulatory G-protein (G_sα), the βγ-subunit of stimulatory G-protein (G_βγ), the adenylyl cyclases of type 5/6 or 4/7 (AC5/6 or AC4/7, respectively), the phosphodiesterases of type 2, 3, or 4 (PDE2, PDE3, or PDE4, respectively), the cyclic AMP (cAMP), regulatory (R) and catalytic (C) subunits of protein kinase A holoenzyme, the protein kinase A inhibitor (PKI), the G-protein-coupled receptor kinase of type 2 (GRK2), the protein phosphatases of type 1 or 2A (PP1 or PP2A, respectively), the inhibitor-1 (I-1). The cytosolic proteins which are the substrates of the β₁-adrenergic signaling system are the phospholamban (PLB) and troponin I (TnI). Stimulatory links are shown by black arrows and inhibitory links are shown by red dashed lines with balls. [Ca²⁺]_i, [Na⁺]_i, and [K⁺]_i are the intracellular Ca²⁺, Na⁺, and K⁺ concentrations in the caveolae, extracaveolae, and cytosol; [Ca²⁺]_o, [Na⁺]_o, and [K⁺]_o are the extracellular Ca²⁺, Na⁺, and K⁺ concentrations.

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Our model cell consists of several compartments (Fig. 1; Appendix S1). For the β₁-adrenergic signaling system we consider three major functional compartments: caveolae (cav), extracaveolae (ecav), and cytosol (cyt) [8], [13]. The caveolae compartment is a submembrane compartment associated with the protein caveolin-3. The extracaveolae compartment is also a submembrane compartment associated with cholesterol-rich lipid rafts, but it does not include caveolin-3. Both caveolae and extracaveolae compartments together represent the particulate fraction. The cytosolic compartment (the soluble fraction) represents the rest of the cell volume, excluding mitochondria. As the dynamics of Ca²⁺ concentration does not directly depend on the β₁-adrenergic signaling system, we use the same compartmentalization of Ca²⁺ handling as in Bondarenko et al. [25]. The subspace volume (V_ss) of the Ca²⁺ handling system is completely located in the extracaveolae compartment of the β₁-adrenergic signaling system.

Total protein concentrations and their activities are normalized to the cell volume as in [8]. In most cases, we used Table 9 from [27] to convert protein concentrations from pmol/mg cell protein to the concentrations in µM. The localization of different signaling proteins and protein kinase A substrates in subcellular compartments can be found in Fig. 1 and Appendix S1 and will be described below in the corresponding chapters. The experimental data in the Methods chapter are used for constraining the model; the experimental data in the Results chapter are used for testing the developed model. The latter experimental data were not used for constraining the model.

In all compartments, the β₁-adrenergic signaling system is activated by agonist (isoproterenol) (Fig. 1). Stimulation of β₁-ARs leads to activation of the stimulatory G protein, G_s, which dissociates into G_sα and G_sβγ subunits. Both subunits activate adenylyl cyclases (AC5/6 or AC4/7, depending on the cellular compartment), which produce cyclic AMP. cAMP is degraded by phosphodiesterases, three isoforms of which, PDE2, PDE3, and PDE4, are included in our model. Balanced activities of ACs and PDEs establish steady-state levels of cAMP in different compartments. cAMP further activates protein kinase A holoenzyme, which consists of two regulatory and two catalytic subunits. Binding four cAMP molecules to PKA holoenzyme causes dissociation of two catalytic subunits that phosphorylate target proteins, among them are PDE3 and PDE4. β₁-ARs are phosphorylated by PKA, as well as by G protein coupled receptor kinase of type 2 (GRK2). PKA is also regulated by heat-stable protein kinase inhibitor (PKI). Intracellular proteins are dephosphorylated by two types of phosphatases, protein phosphatase 1 and 2A. PKA target proteins are located in different compartments. In our model, 20% of the L-type Ca²⁺ channels (the L-type Ca²⁺ current, I_CaL), the fast Na⁺ current, I_Na, and the phospholemman, which regulates the Na⁺-K⁺ pump, I_NaK, are localized in the caveolae compartment; 80% of the L-type Ca²⁺ channels, the ryanodine receptors, RyRs, the ultra-rapidly activating delayed rectifier K⁺ current, I_Kur, the rapidly inactivating transient outward K⁺ current, I_Kto,f, and the time-independent K⁺ current, I_K1, are localized in the extracaveolae compartment; and phospholamban and troponin I are localized in the cytosolic compartment (more details are shown below).

Model Development: Biochemical Part

β₁-adrenergic receptor module.

According to the experimental findings [19], [20], [28], the vast majority of β₁-adrenergic receptors are located in non-caveolae fractions. The estimated total concentration of β₁-ARs in mouse ventricular myocytes is 0.0103 µM [29]. In our model, we distribute the β₁-ARs almost evenly between the extracaveolae and cytosolic compartments, with only 1% located in the caveolae compartment (see Appendix S1). Such distribution of β₁-ARs allowed us to obtain in the model approximately equal cAMP transients in the caveolae and extracaveolae compartments, which is in line with the measurements of local cAMP concentrations in similar compartments in rat and mouse ventricular myocytes [30]. In the β₁-adrenergic receptor module, we separate relatively fast biochemical reactions (ligand-receptor and G-protein-receptor interactions, with time scales of tens milliseconds [31]), which are described by algebraic equations in steady-state approximation, and slower reactions (G-protein activation (hundreds milliseconds [31]), PKA- and GRK2-mediated phosphorylation (hundreds seconds [31]; GRK2, G-protein-coupled receptor kinase of type 2)), which are described by ordinary differential equations (see Appendix S1).

In order to derive algebraic equations which describe ligand-receptor and G-protein-receptor interactions in the caveolae compartment (equations (A.7)-(A.11) in the Appendix S1), we consider mass conservation laws for non-phosphorylated β₁-adrenergic receptors and G-proteins in that compartment:(1)(2)where is the total concentration of non-phosphorylated (np) β₁-ARs in the caveolae compartment, is the concentration of β₁-ARs with bound ligand L (concentration [L]), is the concentration of β₁-ARs with bound ligand L and stimulatory G-protein G_s, is the concentration of β₁-ARs with bound G_s, is the concentration of free β₁-ARs, is the total concentration of the stimulatory G-protein G_s, and is the concentration of free G_s.

Concentrations of complexes , , and can be obtained from the steady-state approximation for corresponding biochemical reactions, provided that the related dissociation constants are known (equations (A.12)-(A.14) in the Appendix S1). The steady-state approximation for a chemical reaction describes the formation of complex AB from the substances A and B: A+B ↔ AB. For this reaction, k⁺ and k⁻ are the forward and backward rates, respectively, and K is the dissociation constant (K = k⁻/k⁺). The complex formation is described by the differential equation d[AB]/dt = k⁺[A]·[B] − k⁻[AB], where [A], [B], and [AB] are the concentrations of the substances A, B, and complex AB, respectively. In steady state, d[AB]/dt = 0, therefore, k⁺[A]·[B] − k⁻[AB] = 0. From the last equation, we can determine the concentration of complex AB in the steady-state approximation: [AB] = [A]·[B]/(k⁻/k⁺) = [A]·[B]/K.

Substitution of the equation for , and into equation (1) and solution with respect to yields equation (A.11). Further substitution of the expressions for , , , and into equation (2) results in equation (A.10). The complete system of algebraic equations for ligand-receptor and G-protein-receptor interactions for the caveolae, extracaveolae, and cytosolic compartments is given in Appendix S1.

Activation of G_s-proteins, with dissociation of and -subunits, occurs through a relatively fast process with complex or a relatively slow process with complex, and is hydrolyzed further to is formed back through re-association of and (equations (A.17)-(A.19) in Appendix S1) [8], [10].

Phosphorylation (desensitization) of β₁-ARs occurs by both protein kinase A and G-protein-coupled receptor kinase of type 2, GRK2 [8], [10] (equations (A.15) and (A.16) for the caveolae compartment). PKA phosphorylates β₁-ARs both in ligand- and G-protein-bound states and unbound states, while GRK2 phosphorylation affects only ligand-bound states [8], [10]. According to the experimental finding [32], application of 10 µM of β₁-ARs agonist isoproterenol increased the phosphorylation level of β₁-ARs by about 108% (Fig. 2), which is reproduced by our model. Moreover, about 30% of phosphorylation of β₁-ARs occurs by GRK2, as it is found from the suppression of PKA by H-89 (Fig. 2). Our model is also able to reproduce this effect.

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Figure 2. β₁-adrenoceptors phosphorylation.

β₁-adrenoceptors phosphorylation above basal level after 15-minute application of 10 µM isoproterenol or 10 µM isoproterenol+PKA inhibitor H-89. Experimental data from Freedman et al. [32] are shown with black bars with errors, simulation data are shown with gray bars. Effect of H-89 was simulated by setting [PKA]_tot = 0 µM.

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Adenylyl cyclase module.

In a β₁-adrenergic pathway, adenylyl cyclases are responsible for synthesis of cAMP from ATP. Our model includes four major types of adenylyl cyclases (AC) found in mouse ventricular myocytes, AC4, AC5, AC6, and AC7 [33], [34]. Two of them, AC5 and AC6, are located in caveolae and have similar properties (we denote them as AC5/6) [35]. Two others, AC4 and AC7, also have similar properties: they do not co-immunoprecipitate with caveolin-3 and they are excluded from caveolae (we denote them as AC4/7) [13], [28], [36].

We simulated activation of adenylyl cyclases by the α-subunit of G-protein, G_sα, [8], [13] (see Appendix S1). In addition, we considered the stimulation of adenylyl cyclases AC5/6 and AC4/7 by βγ-subunit, G_sβγ, according to the experimental data [37], [38], [39], [40]. The total amount of adenylyl cyclases in a cardiac cell is estimated as 0.02622 µM [41], with 74% of AC5/6 type [8].

Figure 3A shows experimental data on activation of AC5 and AC6 by G_sα [37] and corresponding simulation data using our model for AC5/6 activation. In Fig. 3B, simulation data on activation of AC4/7 by G_sα is compared to the experimental data for AC4 [38], [40]. Figures 3C and 3D compare the experimental data from [39], [40] to our simulations for the dependence of AC5/6 and AC4/7 activities on G_sβγ. Both figures show good agreement between the experimental and simulated results.

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Figure 3. Normalized activity of adenylyl cyclases as functions of G_sα and G_sβγ.

Panel A: Experimental normalized activity of AC5 (filled circles) and AC6 (unfilled circles) as functions of G_sα [37]. Simulated data for normalized activity of AC5/6 is shown by a solid line. Panel B: Experimental normalized activity of AC4 (filled circles from [40] and unfilled circles from [38]) as functions of G_sα. Simulated data for normalized activity of AC4/7 is shown by a solid line. Panel C: Experimental normalized activity of AC5 (filled circles) [39] as functions of G_sβγ. Simulated data for normalized activity of AC5/6 is shown by a solid line. Panel D: Experimental normalized activity of AC4 (filled circles) [40] as functions of G_sβγ. Simulated data for normalized activity of AC4/7 is shown by a solid line.

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We also simulated the effects of different concentrations of β₁-adrenoceptor agonist isoproterenol on adenylyl cyclase activity in mouse ventricular myocytes (Fig. 4A). Experimental data on total AC activity in mouse ventricles and cardiac cells as a function of isoproterenol concentration after 10-min exposures are shown by unfilled [42] and filled circles [43] with error bars. Simulation data on AC activity at the 10^th minute after the exposure to different concentrations of isoproterenol are shown by a solid line. As seen in Fig. 4A, our model was able to reproduce absolute values of the total cellular adenylyl cyclase activity as a function of isoproterenol.

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Figure 4. Adenylyl cyclase activity as a function of isoproterenol.

Panel A: Experimental data on AC activity (in pmol/mg/min) in mouse hearts and ventricular myocytes obtained after 10-minutes exposure to isoproterenol are shown by unfilled circles [42] and filled circles [43]. The solid line shows corresponding simulated AC activities at different concentrations of isoproterenol. Panel B: Desensitization of β₁-ARs. Increase in adenylyl cyclase activities above basal level (in %) are measured at maximum (from 50^th to 75^th seconds, control, filled circles) and at two time moments (5 min and 30 min, unfilled circles and unfilled squares, respectively) after exposure to different concentrations of isoproterenol [32]. Corresponding simulated data for the maximum, 5-minute, and 30-minute delays are shown by solid, dashed, and dash-dotted lines, respectively.

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Adenylyl cyclase activity can also be used as an indicator of desensitization of β₁-ARs. Experimental data on AC activity as a function of isoproterenol were obtained by Freedman et al. [32] at three time moments after exposure to an agonist (at the maximum activity (from 50^th to 75^th seconds, depending on isoproterenol concentration), 5^th min, and 30^th min). It is shown that the AC activity decreases in time, reflecting β₁-ARs desensitization (phosphorylation by PKA and GRK2) (symbols in Fig. 4B). Our model satisfactory reproduced this phenomenon. Simulation data also demonstrates the decrease in AC activity as a function of time at different concentrations of isoproterenol (solid, dashed, and dash-dotted lines in Fig. 4B).

Phosphodiesterase module.

Phosphodiesterases in the β₁-adrenergic signaling system degrades cAMP into inert molecule 5′-AMP. We included in our model three major types of phosphodiesterases (PDE2, PDE3, and PDE4) found in mouse ventricular myocytes [44]. While a significant amount of PDE1 was found in mouse ventricles, the study of Bode et al. [45] shows that this type of PDE is predominantly located in non-myocyte cells. As in previous models [8], [13], we put PDE2, PDE3, and PDE4 into the caveolae and cytosolic compartments, and PDE2 and PDE4 into the extracaveolae compartment. Such distribution fits available experimental data on their localization [46], [47]. For subcellular distribution of the PDE isoforms we used experimental data obtained by Mongillo et al. [48] for rat ventricular myocytes, and the parameters were adjusted to fit experimental data on PDE2, PDE3, and PDE4 activities in mouse hearts [44], [49].

PDE2, PDE3, and PDE4 are activated by cAMP molecules, but with different affinities (see Appendix S1). In addition, phosphorylation of PDE3 and PDE4 increases their activities by several folds. These processes are simulated by ordinary differential equations derived for three subcellular compartments (caveolae, extracaveolae, and cytosol, see Appendix S1). Our model also tested the effects of non-specific PDE inhibitor 3-isobutyl-1-methylxanthine (IBMX).

Figure 5A shows experimental and simulated absolute activities of PDE2, PDE3, and PDE4 in mouse and rat hearts. There are some differences in the magnitudes of experimental contributions of different PDE isoforms in total cellular PDE activity obtained by different research groups and between species. However, these differences are diminished in Fig. 5B for fractional contributions of different PDEs and between species. Our model successfully reproduced both absolute PDE activities and the fractional contributions of PDE2, PDE3, and PDE4 to the total cellular PDE activity. In addition to the cellular activity, we were able to reproduce the partial contributions of different PDE isoforms into the total PDE activity of particulate fraction (Fig. 5C). In this figure, we used experimental data of Mongillo et al. [48] obtained from rat cardiomyocytes.

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Figure 5. The effects of β₁-adrenoceptor stimulation on PDE activities.

Panel A: Absolute total PDE activities and the activities of PDE2, PDE3, and PDE4 obtained experimentally from the mouse and rat hearts (in pmol/min/mg protein, bars with errors [44], [49]) and corresponding simulation data (bars without errors). Panel B: Fractional activities of PDE2, PDE3, and PDE4 obtained experimentally from the mouse and rat hearts (in %, bars with errors [44], [49]) and corresponding simulation data (bars without errors). Panel C: Partial activities of PDE2, PDE3, and PDE4 obtained experimentally from the particulate fraction of the rat hearts (in %, bars with errors [48]) and corresponding simulation data (bars without errors). In the experiments and simulations, PDE activities are obtained at fixed cAMP concentrations of 1 µM. Panel D: The effects of PDE inhibitor IBMX on cAMP levels in ventricular myocytes. Experimental data for rat [147] and canine [148] ventricular myocytes are shown by bars with errors, simulation data are shown by bars without errors. In the experiments with rat ventricular myocytes measurements were performed after 3-minute stimulations (5 µM isoproterenol, or 100 µM IBMX, or both) [147]. In the experiments with canine ventricular myocytes measurements were performed after 5-minute stimulations (10 µM isoproterenol, or 10 µM IBMX, or both) [148]. Simulated cAMP level is determined at the 3^rd minute upon application of 5 µM isoproterenol, or 100 µM IBMX, or both.

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The effects of the PDE inhibitor IBMX on cAMP production in ventricular myocytes can be estimated by the levels of cAMP at different experimental conditions. Figure 5D shows experimental cAMP levels in ventricular myocytes from the rat and canine hearts at the resting state after application of isoproterenol or IBMX separately and at simultaneous application of IBMX and isoproterenol. It is remarkable that the experimental data from both species are very similar (bars with the errors in Fig. 5D). Our model reproduces the experimental cAMP level after application of different combinations of IBMX and isoproterenol (bars without errors).

cAMP-PKA module.

cAMP molecules generated in cardiac myocytes by adenylyl cyclases and partially hydrolyzed by phosphodiesterases activate protein kinase A, a major signaling molecule in the β₁-adrenergic signaling system which phosphorylates ion channels and proteins of the Ca²⁺ handling system. Inactive PKA holoenzyme consists of two regulatory subunits R (both either of type I, RI, or type II, RII) and two catalytic subunits C. Activation of PKA holoenzyme requires binding four cAMP molecules, in general, with different affinities. PKA holoenzyme with bound four cAMP molecules dissociates two catalytic subunits, which phosphorylates target proteins. In our model, we consider identical affinities for all four binding sites of PKA. Two isoforms of PKA holoenzyme are found in mouse ventricular myocytes, PKAI and PKAII, which differ by their regulatory subunits. PKAI is predominantly located in the cytosolic compartment, and PKAII is the predominant isoform in the caveolae and extracaveolae compartments.

PKAI and PKAII differ not only by their location, but also by their half-activation constants, K_PKAI and K_PKAII. Some experimental data suggest half-activation constants for K_PKAI ∼ 0.1 µM [50], [51] and K_PKAII ∼ 0.5 µM [51], one of which is significantly smaller and the other is comparable to the resting cAMP concentrations in cardiac cells ∼ 0.5–1 µM [52], [53]. Under such conditions, almost all PKA in the cytosol and most PKA in the caveolae and extracaveolar compartments must be activated. Other experimental data suggest K_PKAI and K_PKAII in the range ∼ 1.5–3 µM [54], [55], [56]. As it was pointed out by Dao et al. [55], relatively small values of K_PKAI and K_PKAII in the nanomolar range were obtained in some experiments because they used free regulatory subunits RI or RII instead of PKA holoenzymes. Experimental data with PKA holoenzymes yielded significantly larger dissociation constants, which are used in our model (K_PKAI,1 and K_PKAI,2 = 2.9 µM [55]; K_PKAII,1 and K_PKAII,2 = 2.5 µM [8], [54]). Activation of PKA holoenzyme is described by ordinary differential equations (see Appendix S1). In addition, the model includes inhibition of PKA by heat-stable protein kinase inhibitor (PKI), the dynamics of which are also described by a differential equation.

Figure 6A shows activation levels of PKAI and PKAII as functions of cAMP concentrations. We used experimental data [54], [55] shown by circles (PKAI) and squares (PKAII). Our simulations are displayed by a solid (PKAI) and a dashed (PKAII) line, respectively. They fit reasonably well to the experimental data. We also simulated the cellular PKA activity ratio in control and upon stimulation of the β₁-adrenergic signaling system by 1 µM isoproterenol (Fig. 6B). Four simulations were performed for this figure: no isoproterenol/basic cAMP level (−cAMP), no isoproterenol/3 µM cAMP (+cAMP), 1 µM isoproterenol/no externally applied cAMP (−cAMP), and 1 µM isoproterenol/3 µM cAMP (+cAMP). Then, the corresponding PKA(−cAMP)/PKA(+cAMP) ratios were calculated. The simulations (grey bars) compare well to the experimental data for the rabbit hearts obtained in control and after application of 1 µM isoproterenol (black bars [57]).

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Figure 6. The effects of β₁-adrenoceptor stimulation on PKA activities.

Panel A: PKA I and PKA II activities as functions of cAMP. Experimental data for PKA I obtained by two methods are shown by filled and unfilled circles [55]; data for PKA II obtained by Beavo et al. [54]. Corresponding simulated data are shown by a solid (PKA I) and a dashed (PKA II) line. Panel B: PKA activity ratio. Experimental data were obtained without (−cAMP) and with (+cAMP) externally applied 3 µM cAMP, both without and with 1 µM isoproterenol (black bars [57]). We also performed four simulations: no isoproterenol/basic level cAMP (−cAMP), no isoproterenol/3 µM cAMP (+cAMP), 1 µM isoproterenol/no externally applied cAMP (−cAMP), and 1 µM isoproterenol/3 µM cAMP (+cAMP). Then, the corresponding PKA ratios were calculated. Panel C: Protein kinase A inhibition by a heat-stable protein kinase inhibitor PKI. Experimentally, PKA activities were measured with and without PKI at different concentrations of cAMP, then their ratio was calculated (in %) and subtracted from 100% (filled circles, [54]). Corresponding simulation data for PKA I and PKA II are shown by solid and dashed lines. Concentration of [PKI]_tot = 2·0.2·[PKA]_tot.

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The effect of a heat-stable protein kinase inhibitor (PKI) on the PKA activity is shown in Fig. 6C. Experimental data obtained from [54] for PKA II are shown by filled circles, and simulation results are plotted by a solid line for PKA I and by a dashed line for PKA II. PKA activities are calculated with and without PKI at different concentrations of cAMP, then their ratios were calculated (in %) and subtracted from 100%. As seen from Fig. 6C, model simulations fit reasonably well to the experimental data.

Protein phosphatases and inhibitor-1 module.

There are two major types of protein phosphatases which are important for cardiac myocyte function, protein phosphatase 1 (PP1) and 2A (PP2A). Localization of PP1 and PP2A in three subcellular compartments can be determined by their co-localization with caveolin-3 and by modulation of their targets. Data of Hescheler et al. [58] and Balijepalli et al. [19] show that the L-type Ca²⁺ current is inhibited by both PP1 and PP2A, and that the portion of the L-type Ca²⁺ channels and PP2A co-localize with caveolin-3, suggesting caveolae localization for both PP1 and PP2A. PP1 and PP2A are also localized in the cytosolic compartment, as they interact with phospholamban and troponin I [59], [60]. In mouse hearts, PP1 is the predominant phosphatase, whose contribution to the total phosphatase activity is ∼75% [61], [62]. As there is no current consensus on whether PP1 or PP2A is predominant in the extracaveolae compartment [63], we assume that only PP1 contributes to phosphatase activity in extracaveolae. We use basically the same molar distribution of PP1 and PP2A in subcellular compartments as Heijman et al. [8] (see Appendix S1), provided that 75% and 25% of cellular phosphatase are of PP1 and PP2A, respectively, as found experimentally in mice [61], [62].

In ventricular myocytes, protein phosphatase 1 is regulated by endogenous inhibitor-1 (I-1) [64]. I-1 is localized in the cytosolic compartment and inhibits PP1 activity when phosphorylated. Cellular concentration of I-1 is estimated as = 0.08543 µM [65]. Ablation of I-1 leads to a moderate increase in PP1 activity and impaired β₁-adrenergic function [64], [65]. As the affinity of I-1 to PP1 is very high (K_Inhib1 = 1 nM), we used steady-state approximation to describe I-1-PP1 interaction with corresponding mass conservation relationships:(3)(4)(5)where is the total concentration of phosphorylated I-1 in cytosol, is the unbound phosphorylated I-1 concentration, is the non-phosphorylated I-1 concentration, is the total concentration of PP1 in cytosol, and is the unbound PP1 concentration. Solution of equations (3) – (5) gives the equations for calculating and (see equations (A.124) – (A.129) in the Appendix S1). Phosphorylation and dephosphorylation of I-1 occurs by the catalytic subunit of PKA and PP2A, respectively [64], [66], and is described by equation (A.130) (see Appendix S1).

Figure 7A shows the effects of activation of the β₁-adrenergic signaling system by 1 µM isoproterenol on inhibitor-1 activity. As there is no data for mice, we used the experimental data from guinea pig hearts [67] which shows significant activation of I-1 from ∼20% to ∼80% of its maximum activity. Our model reproduced the experimental data on I-1 activation. The effects of I-1 on PP1 activity can be estimated from data obtained from WT and I-1 knockout mice [64]. Figure 7B shows a slight increase in PP1 activity upon I-1 ablation (activity of PP1 in I-1 knockout mice is normalized to 100%). In the model, the effect of I-1 knockout is simulated by setting = 0, which leads to a slightly smaller increase in PP1 activity compared to that found experimentally.

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Figure 7. The effects of β₁-adrenoceptor stimulation on activities of I-1 and PP1.

Panel A: Relative I-1 activity in ventricular myocytes in control (left bars) and upon stimulation with 1 µM isoproterenol (right bars). Experimental data for guinea pig hearts [67] are shown by black bars, simulation data with our model are shown by gray bars. Panel B: Relative PP1 activity in WT and I-1 knockout mouse hearts. Experimental data [64] are shown by black bars, our simulations – by gray bars. Experimental PP1 activity from I-1 knockout mouse hearts is normalized to 100%.

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cAMP dynamics.

cAMP is a one of the major signaling small molecules in the β₁-adrenergic signaling system. It moves freely between cellular compartments and has PKA as a major target. cAMP concentration is determined by the balance between cAMP production by adenylyl cyclases, cAMP degradation by phosphodiesterases, and cAMP diffusion between intracellular compartments (caveolae, extracaveolae, and cytosol) (see (A.131)-(A.133) in Appendix S1). Experimental data with unstimulated cells shows cAMP concentrations in mouse ventricular myocytes in the range from 2.4 to 6.0 pmol/mg protein (0.4522–1.13 µM) [43], [52], [53]. Our model gives a background cellular cAMP concentration ∼ 0.3 µM. This concentration is close to the experimental values and to the values obtained in the models of others [8], [11].

Stimulation of the β₁-adrenergic signaling system results in an increase of cAMP production by adenylyl cyclases and cAMP degradation by phosphodiesterases in the caveolae, extracaveolae, and cytosolic compartments. Figure 8A shows experimental time courses of normalized cAMP in mouse [68] and rabbit [57] ventricular myocytes obtained upon stimulation with 1 µM isoproterenol (unfilled and filled circles, respectively). A solid line in Fig. 8A shows corresponding simulated time behavior of cAMP. Both simulated and experimental data show transient increase in cAMP concentration, which is due to changes in cAMP production by adenylyl cyclases, cAMP degradation by phosphodiesterases, cAMP fluxes between compartments, and β₁-ARs desensitization.

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Figure 8. cAMP and PKA dynamics in mouse ventricular myocytes.

Panel A: cAMP dynamics in ventricular myocytes. Experimental data of normalized cAMP in mouse [68] and rabbit [57] ventricular myocytes are shown by unfilled and filled circles, respectively; simulation data is shown by a solid line. Panel B: PKA dynamics in ventricular myocytes. Experimental data of normalized PKA activity in rabbit [57] ventricular myocytes are shown by unfilled circles; simulation data is shown by a solid line. Data in Panels A and B was obtained upon application of 1 µM isoproterenol.

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PKA dynamics.

Our model is able to reproduce the time course of the cellular PKA activity, which is determined by the cellular concentration of catalytic subunit (solid line in Fig. 8B). As there is no data for mice, we used data of Buxton and Brunton [57] (unfilled circles in Fig. 8B) obtained for rabbit ventricular myocytes to constrain the model. Similar to cAMP dynamics, both experimental and simulation data for PKA demonstrate transient increase in activation, with subsequent decrease in activity.

Model Development: Electrophysiological Part

Electrical activity of the mouse ventricular myocytes is described by the equation for transmembrane potential [25]:where I_CaL is the L-type Ca²⁺ current, I_p(Ca) is the sarcolemmal Ca²⁺ pump, I_NaCa is the Na⁺/Ca²⁺ exchanger, I_Cab is the Ca²⁺ background current, I_Na is the fast Na⁺ current, I_Nab is the Na⁺ background current, I_NaK is the Na⁺-K⁺ pump, I_Kto,f is the rapidly recovering transient outward K⁺ current, I_K1 is the time-independent K⁺ current, I_Kur is the ultrarapidly activating delayed rectifier K⁺ current, I_Kss is the noninactivating steady-state voltage activated K⁺ current, I_Kr is the rapid delayed rectifier K⁺ current, I_Cl,Ca is the Ca²⁺-activated chloride current, and I_stim is the stimulus current.

In our model, we consider four of these currents (I_CaL, I_Na, I_Kto,f, and I_Kur) as the substrates of the β₁-adrenergic signaling system. The Na⁺/K⁺ pump is affected by β₁-ARs through phosphorylation of phospholemman. One more current, I_K1, is also affected by β₁-ARs; however, in the voltage range from about −80 to +40 mV, this current does not change significantly. In addition, there are three other phosphorylation substrates, which are the major players in Ca²⁺ dynamics and are affected by β₁-ARs: ryanodine receptors, phospholamban, and troponin I. We consider all these β₁-adrenoceptor substrates below as separate modules in the model.

L-type Ca²⁺ current module.

As found experimentally, the L-type Ca²⁺ channels are localized in both the caveolae and the extracaveolae compartments [19], [21], [22], [69]. About 80% of the L-type Ca²⁺ channels are found within Ca²⁺ release units, or couplons [21], which are localized in the extracaveolae compartment, contribute directly to excitation-contraction coupling, and are the targets of the β₁-adrenergic signaling system [22], [70]. The other 20% of the L-type Ca²⁺ channels are found in the caveolae [19], [22]. The total amount of L-type Ca²⁺ channel protein can be estimated from the experimental data on the amount of RyRs in the mouse hearts (1058±45 fmol/mg protein, or 0.1993 µM [71]) and dihydropyridine (DHPR) receptor-to-RyRs ratio for rats (RyR/DHPR = 7.3 [72]), resulting in [I_CaL]_tot = 0.0273 µM. In the presented model, 20% and 80% of the L-type Ca²⁺ channels are localized in the caveolae and the extracaveolae compartments, respectively.

Effects of the β₁-adrenergic signaling system on the L-type Ca²⁺ channels and channel gating can be described with a Markov model for non-phosphorylated and phosphorylated states (Fig. 9A). The model includes two activation pathways: one for non-phosphorylated and one for phosphorylated channels. Each pathway includes five closed, one open, and three inactivated states. Transitions between non-phosphorylated and phosphorylated states are determined by the rates of phosphorylation by PKA and dephosphorylation by PP1 and PP2A (see Appendix S1). As we were unable to reproduce the experimental data on isoproterenol effects on the L-type Ca²⁺ channels with the Markov model from [25], [26] due to the high maximum opening probability for the channels at large depolarizations, we introduced a voltage-independent rate limiting step and a new closed state (C_P, closed pre-open state) in the new model (Fig. 9A), which reduced the opening probability for non-phosphorylated channels compared to the models of Bondarenko et al. [25] and Petkova-Kirova et al. [26]. Experimental data shows that the stimulation of β₁-ARs increases the magnitude of the L-type Ca²⁺ current and causes a hyperpolarization shift in normalized channel conductance (G/G_max) and a steady-state inactivation relationship in mouse ventricular myocytes [73], [74], [75]. These effects are simulated by several changes to the phosphorylated pathway in the model (see Appendix S1) and an increase in G_CaLp (G_CaLp = 2.09G_CaL according to the estimation of an increase in maximum opening probability for cardiac Ca²⁺ channels from [76]).

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Figure 9. The effects of β₁-adrenoceptor stimulation on the L-type Ca²⁺ current.

Panel A: Markov model of the L-type Ca²⁺ channel. State diagram consists of two similar sub-diagrams for non-phosphorylated (upper sub-diagram) and phosphorylated states (lower sub-diagram). C₁, C₂, C₃, C₄, and C_P are closed states; O is the open state; I₁, I₂, and I₃ are inactivated states; C_1p, C_2p, C_3p, C_4p, and C_Pp are closed phosphorylated states; O_p is the open phosphorylated state; and I_1p, I_2p, and I_3p are phosphorylated inactivated states. The rate constants α, α_p, and β are voltage-dependent; γ is calcium dependent; k_co, k_oc, k_cop, K_pcf and K_pcb, are voltage-insensitive; and k_phos and k_dephos are the phosphorylation and dephosphorylation rates, respectively (see Appendix S1). Panel B: Time course of the peak values of L-type Ca²⁺ current and L-type Ca²⁺ channel phosphorylation level upon stimulation with 1 µM isoproterenol. Experimental data for peak I_CaL is obtained by a series of pulses to 0 mV for 200 ms from a holding potential of −80 mV with a frequency 0.2 Hz [75]. Modeling data are obtained by a series of pulses to 0 mV for 50 ms from a holding potential of −80 mV with a frequency 0.04 Hz. Increase in phosphorylation level is determined as a fractional increase related to the total increase in phosphorylation of L-type Ca²⁺ channels at 150^th s after application of isoproterenol. Panel C: Peak L-type Ca²⁺ current as a function of isoproterenol concentration. Experimental data are obtained by Kim et al. [79] (filled circles), Sako et al. [80] (unfilled circles), and Mitarai et al. [81] (filled squares). Simulation data is obtained by a voltage pulse to 0 mV from a holding potential of −80 mV after a 600-second exposure to different concentrations of isoproterenol. Simulation data for the total cellular I_CaL,tot, the caveolae-localized I_CaL,cav, and the extracaveolae-localized I_CaL,ecav are shown by black, green, and red solid lines, respectively. Panel D: Simulated time course of the L-type Ca²⁺ currents in control (solid line), after 1000-s exposure to PP1/PP2A inhibitor Calyculin A (65% of PP1/PP2A activity inhibition, dashed line), and after 600-s exposure to 1 µM isoproterenol (dotted line). Currents are obtained by a voltage pulses to 0 mV from a holding potential of −80 mV and without Ca²⁺-induced Ca²⁺ release to account for heavy buffer conditions. Insert in Panel D: Same simulations performed with intact Ca²⁺-induced Ca²⁺ release. Panel E: Peak current-voltage (I–V) relationships for I_CaL in control (filled circles) and after exposure to Calyculin A (unfilled circles) and isoproterenol (filled squares). Panel F: Steady-state inactivation relationships for I_CaL in control (filled circles) and after exposure to Calyculin A (unfilled circles) and isoproterenol (filled squares). Panel G: Normalized maximum conductance (G/G_max) for I_CaL as functions of voltage in control (filled circles) and after exposure to Calyculin A (unfilled circles) and isoproterenol (filled squares). In Panels E, F, and G, currents are obtained by the two-pulse protocols: a 500-ms depolarizing first pulse to between −70 and +50 mV (in 10-mV increment) is applied from a holding potential of −80 mV; this is followed by a second 500-ms pulse to +10 mV. Simulations are performed without Ca²⁺-induced Ca²⁺ release to account for heavy buffer conditions.

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Model parameters are adjusted to fit experimental data on both the basal L-type channel phosphorylation level and the time course of the current amplitude upon stimulation with isoproterenol. Experimental data suggest the basal phosphorylation level of the L-type Ca²⁺ channels in ventricular myocytes to be about 13–20% [77], [78]. In our model, a fraction of phosphorylated channels under basal conditions is set to 10.3%. Upon application of 1 µM isoproterenol, peak values of I_CaL increase in time upon stimulation with voltage pulses to 0 mV, as is seen from the experimental data [75] (Fig. 9B). Our model reproduced the time course of the peak current increase under similar stimulations (solid line in Fig. 9B). It is remarkable that the simulated time course of the peak current increase (solid line in Fig. 9B) is very similar to the simulated time course of the relative phosphorylation level of the L-type Ca²⁺ channels (dashed line in Fig. 9B).

In addition to the time course of I_CaL increase, we simulated magnitudes of I_CaL increase after a 600-second exposure to different concentrations of isoproterenol (Fig. 9C). We evaluated the effects of isoproterenol on the total I_CaL (I_CaL,tot, black bold solid line in Fig. 9C) as well as on I_CaL populations localized in the caveolae (I_CaL,cav, green line in Fig. 9C) and extracaveolae (I_CaL,ecav, red line in Fig. 9C) compartments. The results of simulations for the total I_CaL are in a good agreement with the experimental data obtained by Kim et al. [79], Sako et al. [80], and Mitarai et al. [81] (Fig. 9C). Simulations also show that the effects of β₁-adrenergic receptor agonist is significantly stronger on the channels localized in the extracaveolae compartment (2.03 folds at 1 µM Iso) compared to the channels in the caveolae compartment (1.42 folds at 1 µM Iso). If the caveolae-located I_CaL is responsible for ∼20% of the total current amplitude in control, after exposure to isoproterenol (1 µM) this fraction decreases to ∼15%. The results of simulations are in line with the experimental data of [70] who have shown that the I_CaL from the population of channels in the caveolae compartment comprises about 15% of the total current.

In addition to the effects of activation of the β₁-adrenergic signaling system, our model is tested in respect to the effects of inhibition of phosphatase activity on the L-type Ca²⁺ current. Figure 9D shows simulated I_CaL traces under heavy buffer conditions (with suppression of Ca²⁺-induced Ca²⁺ release) elicited by voltage pulses to 0 mV in control (solid line) and after 1000-s exposure to 1 µM Calyculin A (dashed line) and 600-s exposure to 1 µM isoproterenol (dotted line). In simulations, we consider that Calyculin A inhibits 65% of the activity of both PP1 and PP2A. As seen from simulations in Fig. 9D, both isoproterenol and Calyculin A increase peak currents to different degrees, suggesting that both activation of PKA and inhibition of PP1 and PP2A increase the L-type Ca²⁺ current. Fitting simulated time courses from Fig. 9D yields bi-exponential inactivation of I_CaL with two time constants. Fast (Ca²⁺-dependent inactivation) and slow (voltage-dependent inactivation) time constants are equal to 7.77 and 22.0 ms, 7.19 and 19.9 ms, and 6.54 and 18.5 ms for control (solid line), after 1000-s exposure to 1 µM Calyculin A (dashed line), and 600-s exposure to 1 µM isoproterenol (dotted line), respectively. These data show significant increase in Ca²⁺-dependent inactivation of I_CaL upon stimulation of the β₁-adrenergic signaling system. Similar behavior of I_CaL is also observed experimentally with BAPTA in pipette solution [73]. Insert in Fig. 9D shows similar simulations with intact Ca²⁺-induced Ca²⁺ release. In the last case, current traces also show bi-exponential decay with the fast and slow time constants 4.83 and 12.4 ms, 4.72 and 12.0 ms, and 4.66 and 12.8 ms for control (solid line), after 1000-s exposure to 1 µM Calyculin A (dashed line), and 600-s exposure to 1 µM isoproterenol (dotted line), respectively. These data show significant increase in the L-type Ca²⁺ current inactivation with intact Ca²⁺ dynamics. Simulations also show that activation of β₁-ARs increases peak current amplitudes by about two-fold (Fig. 9E) and causes a hyperpolarization shift in steady-state inactivation relationships (Fig. 9F) and more moderately in G/G_max data (Fig. 9G). Inhibition of PP1 and PP2A produced an intermediate effect on the I_CaL in terms of an increase in amplitude and a hyperpolarization shift of steady-state inactivation relationships and G/G_max. Similar increases in amplitudes and hyperpolarization shifts are also observed experimentally [73]. Therefore, our model for the β₁-adrenergic signaling system is able to simulate the effects of both activation of PKA and inhibition of PP1 and PP2A on the L-type Ca²⁺ current, I_CaL.

Fast Na⁺ current module.

The channels responsible for the fast Na⁺ current, I_Na, which are encoded by Nav1.5 subunit, are found in the caveolae compartment [16], [69], [82]. Using both immunoblot analysis and imaging technique, Yarbrough et al. [82] provided evidence of co-localization of the fast Na⁺ channels and caveonin-3 in rat cardiomyocytes, suggesting their localization in the caveolae compartment. Similar data were also obtained by Shibata et al. [69] by using immunogold labeling of plasma membranes from rat cardiomyocytes, where Nav1.5 subunits were co-localized on electron microscope images with caveolin-3. In addition, Palygin et al. [83] provided evidence of the involvement of caveolin-3 in isoproterenol-induced enhancement of I_Na in ventricular myocytes.

Activation of the β₁-adrenergic signaling system with isoproterenol leads to an increase in the amplitude of I_Na, however, without the effects on gating properties of the channel [84], [85]. Simultaneous activation of several components of the β₁-adrenergic signaling system with cAMP-IBMX-forskolin cocktail or with excessive application of membrane permeant analogue of cAMP, CPTcAMP (5 mM), results in additional small shift in the G/G_max and steady-state inactivation [86], [87], [88]. Experimental data of Baba et al. [86] also shows that the inhibition of protein phosphatase PP2A causes an increase in I_Na, and the addition of PP2A to pipette solution causes a decrease in I_Na, which link phosphorylation level of I_Na to its magnitude. Mechanism of the changes in I_Na was studied by Zhou et al. [88] in detail. It was shown that, in addition to channel phosphorylation, an increased number of functional fast Na⁺ channels in the cell membrane is due to the channel trafficking. More recent analysis of the effects of PKA on I_Na suggested that phosphorylation and trafficking of I_Na are related processes: channels’ phosphorylation increases trafficking of fast Na⁺ channels [89].

To simulate these effects, we developed a Markov model for I_Na, based on the model [25], [90], in a similar way as for I_CaL, but with some differences. We consider that the amplification of I_Na occurs through two processes: phosphorylation of the channels and their subsequent trafficking to the cell membrane. As the kinetics of the two processes are indistinguishable in the experiments, we use only one rate constant to characterize the effect of PKA, k_phos,tr, which includes both channel’s phosphorylation and trafficking. Two activation pathways are used, one is for non-phosphorylated channels and another is for phosphorylated-trafficked channels (Fig. 10A). Because isoproterenol does not change the gating properties of I_Na, we use the same rate constants for both non-phosphorylated and phosphorylated-trafficked channels. The larger conductance is used for the phosphorylated-trafficked channels (see the fast Na⁺ current module in Appendix S1). We consider that the fast Na⁺ channels are dephosphorylated by PP1 and PP2A (Fig. 10A, Appendix S1). The set of equations that describes the fast Na⁺ channel gating is provided in Appendix S1 ((A.180) - (A.213)).

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Figure 10. The effects of β₁-adrenoceptor stimulation on the fast Na⁺ current.

Panel A: Markov model of the fast Na⁺ channel. State diagram consists of two similar sub-diagrams for non-phosphorylated (upper sub-diagram) and phosphorylated-trafficked states (lower sub-diagram). C_Na1, C_Na2, and C_Na3 are closed states; O_Na is the open state; IF_Na, I1_Na, and I2_Na are the fast, intermediate, and slow inactivated states, respectively; IC_Na2 and IC_Na3 are closed-inactivated states; C_Na1p, C_Na2p, and C_Na3p are closed phosphorylated states; O_Nap is the open phosphorylated state; and IF_Nap, I1_Nap, I2_Nap, IC_Na2p, and IC_Na3p are phosphorylated inactivated states. The rate constants for activation, deactivation, inactivation, phosphorylation-trafficking, and dephosphorylation are given in Appendix S1. Panel B: Time course of the activation of the fast Na⁺ current upon application 0.1 µM isoproterenol. Experimental data of Matsuda et al. [85] obtained for the normalized peak I_Na in rabbit ventricular myocytes is shown by closed circles. Data is obtained with 40-ms pulses from a holding potential of −100 mV to −30 mV at stimulation frequency 0.2 Hz. A solid line shows the time course of simulated data on relative I_Na phosphorylation upon application of 0.1 µM isoproterenol. A dashed line shows the time course of the simulated normalized peak I_Na after application of 0.1 µM isoproterenol. The simulated currents are obtained with 20-ms pulses from a holding potential of −140 mV to −30 mV at stimulation frequency 0.04 Hz. Panel C: An increase in peak I_Na availability upon application of different concentrations of isoproterenol (in %). Experimental data by Kirstein et al. [84] obtained from rat ventricular myocytes are shown by black bars with errors; corresponding simulation data are shown by gray bars. Peak current-voltage (Panel D) and steady-state inactivation (Panel E) relationships for the fast Na⁺ current in ventricular myocytes upon stimulation with 0.1 µM isoproterenol. Experimental data for rats in the absence (unfilled circles) and presence (filled circles) of 0.1 µM isoproterenol are obtained by Kirstein et al. [84] (holding potential is −100 mV, conditioning pulse duration is 2,500 ms; isoproterenol data is obtained after 10 min of application). Simulated data are shown by solid (no isoproterenol) and dashed (10 min after application of 0.1 µM isoproterenol) lines (data are obtained by two-pulse protocol, holding potential is −140 mV, first pulse duration is 500 ms for voltages from −140 to +40 mV in 10 mV steps, second pulse duration is 50 ms at voltage −20 mV). Isoproterenol increases I_Na availability, but does not affect gating properties.

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The resulting model for the fast Na⁺ current was tested against the experimental data on the time course of I_Na activation, its dependence on the isoproterenol concentration, and voltage-clamp experiments (Fig. 10). As there is no data for mice, we used the experimental time course of the activation of I_Na by 0.1 µM isoproterenol obtained from rabbit ventricular myocytes (filled circles in Fig. 10B). Figure 10B shows a good agreement between the experimental and simulated time dependences of I_Na amplitude upon stimulation of the β₁-adrenergic signaling system. A similar time course is demonstrated by the simulated fraction of phosphorylated and trafficked Na⁺ channels (solid line in Fig. 10B). The model also successfully reproduced the concentration dependence of an increase in Na⁺ channel availability at different concentrations of isoproterenol (Fig. 10C).

Experimental data shows an increase in the fast Na⁺ current amplitude upon stimulation with 0.1 µM isoproterenol (Fig. 10D, unfilled and filled circles). A similar increase is obtained from our Markov model for Na⁺ channels (solid and dashed lines in Fig. 10D are for control and 0.1 µM isoproterenol, respectively). Neither the experimental data (unfilled and filled circles in Fig. 10E) nor the simulations (solid and dashed lines in Fig. 10E) demonstrate significant changes in steady-state inactivation relationships.

Ryanodine receptor module.

Experimental studies of ryanodine receptors in rat ventricular myocytes provided evidence of their co-localization in couplons with the L-type Ca²⁺ channels (in dyads, or subspace volume V_ss) or in close proximity to those couplons [21], [22], [91]. Between 80 to 85% of ryanodine receptors are localized in V_ss and the rest are very close to dyads, which suggests their involvement in Ca²⁺-induced Ca²⁺ release [21], [91]. Very small portions (∼3.5–9.2%) of ryanodine receptors in mouse ventricular myocytes are shown to co-localize with caveolin-3, but outside of couplons, but their functional significance is unclear [35], [92]. Therefore, in the model, we put ryanodine receptors in the extracaveolae compartment. The receptors are subjects of phosphorylation by PKA and dephosphorylation by PP1. The total concentration of RyRs in mouse ventricular myocytes was determined experimentally by Chu et al. [71] and is equal to 0.1993 µM.

A Markov model for ryanodine receptor gating, which includes phosphorylation-dephosphorylation processes, is shown in Fig. 11A. As for two other substrates, I_CaL and I_Na, we developed a Markov model that consists of two populations of the channels, non-phosphorylated and phosphorylated. For non-phosphorylated channels, we employed our previously developed Markov model for RyRs, which contains two closed (C₁ and C₂) and two open (O₁ and O₂) states [25]. We added two closed-phosphorylated (C_1p and C_2p) and two open phosphorylated (O_1p and O_2p) states to the model and the transitions between corresponding non-phosphorylated and phosphorylated states (Fig. 11A). Because experimental data suggest slightly increased sensitivity of RyRs to cytosolic Ca²⁺ concentration [93], we sped up the forward transition rates to a greater magnitude than the backward transition rates for the phosphorylated channels (see Appendix S1). Differential equations, which describe the time behavior of the RyRs’ probabilities in closed and open states, are shown in Appendix S1 (Eqs. (A.214)-(A.222)).

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Figure 11. The effects of β₁-adrenoceptor stimulation on ryanodine receptors.

Panel A: Markov model of ryanodine receptors. State diagram consists of two similar sub-diagrams for non-phosphorylated (upper sub-diagram) and phosphorylated states (lower sub-diagram). C₁ and C₂ are closed states; O₁ and O₂ are open states; C_1p and C_2p are closed phosphorylated states; O_1p and O_2p are open phosphorylated states. The rate constants from C₁ to O₁, from O₁ to O₂, from C_1p to O_1p, and from O_1p to O_2p are Ca²⁺-dependent; and k_phos and k_deph are the phosphorylation and dephosphorylation rates, respectively (see Appendix S1). Panel B: Time course of the relative phosphorylation level of RyRs upon activation of the β₁-adrenergic signaling system. Experimental data of Xiao et al. [94] (filled circles) are obtained upon stimulation of rat ventricular myocytes with 1 µM isoproterenol; experimental data of Takasago et al. [95] (filled squares) are obtained from canine ventricular myocytes with endogenous PKA by application of [γ-³²P]ATP. Modeling data are obtained by application of 1 µM isoproterenol. Increase in phosphorylation level is determined as a fractional increase related to the maximum increase in phosphorylation of RyRs after activation of the β₁-adrenergic signaling system. Panel C: Relative phosphorylation level of RyRs at different concentrations of isoproterenol. Experimental data of Xiao et al. [94] (filled circles) obtained upon stimulation of rat ventricular myocytes for 15 minutes. Simulation data are obtained after 10-minute exposure to different concentrations of isoproterenol. Panel D: Effects of PKA on opening probability of RyRs as function of cytosolic Ca²⁺ concentration. Experimental data of Xiao et al. [93] are obtained for cardiac RyRs upon application of active (filled circles) and boiled (unfilled circles) PKA at relatively small luminal Ca²⁺ of 45 nM; experimental data of Xiao et al. [96] (filled squares) for RyRs are obtained from mouse ventricular myocytes. Simulation data for mouse ventricular myocytes in the absence and presence of PKA are obtained at intracellular [Ca²⁺]_i concentration ranged from 0.01 to 10 µM and are shown by dashed and solid lines. Experimental data obtained at small luminal Ca²⁺ concentration shows larger sensitivity of RyRs to cytosolic Ca²⁺.

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Our model successfully reproduced the time course of the ryanodine receptor phosphorylation upon stimulation of β₁-adrenoceptors. Figure 11B shows experimental time behavior of the relative phosphorylation level of RyRs in rat ventricular myocytes during exposure to 1 µM isoproterenol [94]. A similar time course is demonstrated by our model (solid line in Fig. 11B) and by the experimental data which used a different technique of RyR phosphorylation (by endogenous PKA in canine ventricular myocytes upon application of [γ-³²P]ATP [95]). Figure 11C (filled circles) shows experimental data on the phosphorylation level of RyRs at different concentrations of isoproterenol [94]. Our model is able to reproduce this dependence as well (solid line in Fig. 11C).

In addition, the model simulated dependence of the RyRs open probability as a function of intracellular Ca²⁺ concentration for non-phosphorylated and phosphorylated channels (Fig. 11D). The experimental data on the effects of PKA on RyRs shows a tiny shift of the dependence of phosphorylated RyRs’ opening probability towards a smaller cytosolic Ca²⁺ concentration [93]. However, such data were obtained at relatively small luminal Ca²⁺ concentrations (45 nM), which increased sensitivity of RyRs by an order of magnitude compared to normal physiological conditions (compare the data shown by filled and unfilled circles (small luminal Ca²⁺ concentrations) with the data shown by filled squares (normal physiological luminal Ca²⁺ [96])). To estimate the effects of PKA on RyRs, we simulated two dependences of RyRs opening probabilities on cytosolic Ca²⁺: the first is obtained by stimulation of the cell with intact PKA (solid line in Fig. 11D), the second is obtained by setting [PKA]_tot = 0 µM. Our model shows a reasonable agreement of the Ca²⁺-dependence of the RyRs opening probability with the experimental data [96], but virtually no change in the sensitivity of phosphorylated RyRs to cytosolic Ca²⁺ concentration. Some deviations between the experimental (filled squares) and simulated (solid line) data at relatively large cytosolic Ca²⁺ concentrations can be due to the method of estimation of the opening probabilities: in the simulations, we used the maximum values of the channel’s opening probabilities, without consideration of the effects of ryanodine receptor inactivation, while in the single-channel experiments, such inactivation is always present and can potentially reduce measured opening probability.

Phospholemman and the Na⁺-K⁺ pump module.

Experimental data on the localization of the Na⁺-K⁺ pump shows that ∼30–40% of α₁-subunits and 80–90% of β₁-subunits are localized in the caveolae-rich membrane fractions [97]. Another study provided similar data on the Na⁺-K⁺ pump and caveolin-3 co-localization, where ∼70% of those proteins are found in the same fractions [98]. Moreover, almost all the Na⁺-K⁺ pump activity was found in caveolae [97], [99].

In our model, the phospholemman, which regulates the Na⁺-K⁺ pump, is the third substrate of the β₁-adrenergic signaling system located in the caveolae compartment. Activation of β₁-ARs increases the function of the Na⁺-K⁺ pump by phosphorylation of phospholemman (PLM) through the effective change in dissociation constant K_m,Nai [12], thereby decreasing intracellular [Na⁺]_i concentration [100]. An experimental time course of a relative decrease in [Na⁺]_i in mouse ventricular myocytes after application of 1 µM isoproterenol is shown in Fig. 12A by filled circles. A corresponding simulated time course of a relative PLM phosphorylation level is shown by a solid line. An increase in the phosphorylation level of PLM decreases the Na⁺ half-saturation constant for the current and effectively increases the pumping rate of Na⁺ outside the cell. Both time dependences demonstrate similar behavior.

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Figure 12. The effects of β₁-adrenoceptor stimulation on the Na⁺-K⁺ pump.

Panel A: Experimental time course of a relative decrease in the intracellular [Na⁺]_i concentration (filled circles) obtained by Despa et al. [100] from mouse ventricular myocytes after application of 1 µM isoproterenol and corresponding simulated time course of an increase in relative phosphorylation level of phospholemman obtained using our model (solid line). Panel B: Experimental data on a relative increase in I_NaK current (filled circles) obtained by Gao et al. [101] from guinea pig ventricular myocytes at different concentrations of isoproterenol. Corresponding simulation data with our model on a relative increase in phosphorylation of phospholemman is shown by a solid line. Panel C: Experimental (black bars with errors [100]) and simulated (gray bars) data on intracellular [Na⁺]_i concentration before (control) and after 10-minutes application of 1 µM isoproterenol (Iso).

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Figure 12B shows the experimental dependence of the relative increase in I_NaK as a function of isoproterenol concentration obtained from guinea pig ventricular myocytes (filled circles [101]). We compared the experimental data to our simulations of a relative increase in the phosphorylation level for phospholemman (solid line in Fig. 12B). In general, simulation data has a dependence on isoproterenol concentration similar to the experimental data, except for a point at 0.01 µM isoproterenol. Such deviation could be due to the species differences.

Finally, our model successfully reproduced the experimental behavior of intracellular [Na⁺]_i concentration in mouse ventricular myocytes measured before and 10 minutes after an application of 1 µM isoproterenol (Fig. 12C, [100]). Both the experimental and simulation data show relatively small, but significant decreases in [Na⁺]_i after stimulation of the β₁-adrenergic signaling system.

Ultra-rapidly activating delayed rectifier K⁺ current module.

The ultra-rapidly activating delayed rectifier K⁺ current, I_Kur, is the substrate of PKA in the extracaveolae compartment in cardiomyocytes [15], [102]. I_Kur is predominantly encoded by Kv1.5 channels [103]. It is also localized mostly in lipid rafts, which lack caveolin-3 [104], pointing to the extracaveolae compartment (however, see also [105], [106], where localization of Kv1.5 channels is debated). Similar to the Heijman et al. model [8], we put the I_Kur current in the extracaveolae compartment.

Stimulation of β₁-ARs increases the function of I_Kur [107]. Figure 13A show an experimental time course of I_Kur activation in human atrial myocytes upon application of 1 µM isoproterenol (solid lines with circles, [107]). We adjusted model parameters and performed simulations to fit the experimental time behavior (solid line in Fig. 13A). Our model also reproduced an increase in I_Kur at different concentrations of isoproterenol (Fig. 13B). The saturation of the current amplitude found experimentally is observed at isoproterenol concentrations of 0.1 to 1 µM (solid lines with circles [108]). Similar data is obtained from simulations (solid line in Fig. 13B).

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Figure 13. The effects of β₁-adrenoceptor stimulation on I_Kur and I_Kto,f.

Panel A: Experimental time course of the relative increase in the ultra-rapidly activating delayed-rectifier K⁺ current I_Kur obtained by Li et al. [107] from human atrial myocytes after application of 1 µM isoproterenol (line with filled circles) and corresponding simulated time course of an increase in I_Kur obtained with our model (solid line). Simulation data is obtained with 200-ms pulses from a holding potential of −100 mV to +40 mV at stimulation frequency 0.02 Hz. Panel B: Experimental data on a relative increase in I_Kur current (filled circles) obtained by Yue et al. [108] from canine atrial myocytes at different concentrations of isoproterenol. Corresponding simulation data with our model on relative increase in I_Kur are shown by a solid line. Simulation data is obtained with 4.5-s pulses from a holding potential of −90 mV to 0 mV after 800-s exposure to different concentrations of isoproterenol. Panel C: Experimental (human atrial myocytes [107], solid lines with circles) and simulated (solid and dashed lines) data on current-voltage relationships for I_Kur current. Experimental data for control conditions and those obtained after application of 1 µM isoproterenol are shown by unfilled and filled circles, respectively. Simulated data for control conditions are shown by a solid line, and 1 µM isoproterenol simulations are shown by a dashed line. Simulated currents are obtained by 4.5-s depolarizing pulses to between −80 and +50 mV (in 10-mV increment) from a holding potential of −90 mV. Panel D: Experimental time course of the relative decrease in the rapidly recovering transient outward K⁺ current I_Kto,f obtained by Zhang et al. [111] from mouse Schwann cells after application of 1 µM forskolin (filled circles) or 10 µM db-cAMP (unfilled circles), and corresponding simulated time course of a relative decrease in I_Kto,f phosphorylation obtained with our model after stimulation with 10 µM isoproterenol (solid line). Panel E: Simulated time course of I_Kto,f traces obtained by depolarization pulses to −5 mV from a holding potential of −100 mV for control (solid line) and after stimulation with 10 µM isoproterenol (dashed line). Panel F: Simulated data for G/G_max (black lines) and steady-state inactivation relationships (gray lines) obtained for I_Kto,f with two-pulse protocol (P1 stimuli from −100 to +50 mV in 10 mV intervals for 500 ms, following P2 pulse to +50 mV for 500 ms; holding potential is −100 mV) in control (solid lines) and after application of 10 µM isoproterenol (dashed lines).

https://doi.org/10.1371/journal.pone.0089113.g013

Experimental voltage dependence of the peak ultra-rapidly activating delayed rectifier K⁺ current in response to depolarizations in the interval from −40 to +50 mV for control conditions and after application of 1 µM isoproterenol is shown in Fig. 13C [107]. As in [25], simulated data show activation of I_Kur at slightly more hyperpolarized potentials to offset the effects of divalent cations, which are used in the experiments to block I_CaL. However, both simulated and experimental data show similar increases in peak current amplitude upon stimulation of β₁-ARs (solid and dashed lines in Fig. 13C).

Rapidly recovering transient outward K⁺ current module.

The other substrate of PKA in the extracaveolae compartment in our model is the rapidly recovering transient outward K⁺ current, I_Kto,f. I_Kto,f is found in lipid rafts that lack caveolin-3 pointing to non-caveolae localization [15], [69], [105]. Heijman et al. [8] also placed I_to1, which is encoded by Shal-type K⁺ channels (Kv4.2/Kv4.3), to the extracaveolae compartment.

There are only a few qualitative experimental data on the effects of activation of the β₁-adrenergic signaling system on I_Kto,f in cardiac cells [109]. Experimental data of Gonzalez de la Fuente et al. [109] shows clear inhibition of I_to1 by isoproterenol (0.1 µM) in human left and right atrial myocytes by about 40–50%. Similar inhibition is obtained in neural cells [110] for A-type K⁺ current, I_A, which is also encoded by Shal-type K⁺ channels (Kv4.2), after application of 8-br-cAMP (100 µM), and Schwann cells [111] after application of bradykinin (5 µM), forskolin (1 µM), or db-cAMP (10 µM). Our simulation data shows about a two-fold decrease in peak I_Kto,f at saturating concentrations of isoproterenol (Fig. 13E).

Figure 13D shows experimental time courses of I_A-current inhibition by forskolin (1 µM) or db-cAMP (10 µM) obtained in Schwann cells [111] (filled and unfilled circles, respectively). Our simulation, shown by a solid line for the saturating concentration of isoproterenol (10 µM), gives a reasonable agreement with the experimental data. The saturating concentration of isoproterenol was chosen in the simulation to obtain cAMP concentration in the extracaveolae compartment similar to the experimental values and maximum activation of PKA.

Simulated time courses of I_Kto,f in control and after application of 10 µM isoproterenol are shown in Fig. 13E by solid and dashed lines, respectively. Calculations demonstrate about a two-fold inhibition of peak current after stimulation of β₁-ARs. A similar level of inhibition of I_A is obtained by activation of PKA with saturating concentrations of 8-br-cAMP (100 µM) in neural cells [110], and I_to1 after application of saturating concentrations of isoproterenol in human left and right atrial cells [109]. Simulations also demonstrate depolarization shifts in voltage dependences of G/G_max (13 mV) and steady-state inactivation (6 mV) for isoproterenol-stimulated compared to control cells (Fig. 13F), which is similar to the experimental data from [110] obtained for neural cells.

Time-independent K⁺ current module.

While experimental data shows the effects of activation of the β₁-adrenergic signaling system on the time-independent current I_K1, such effects are clear only at potentials below −80 mV [112], [113]. Therefore, we did not include modulation of I_K1 by β₁-ARs in our model.

Phospholamban module.

Phospholamban is the first PKA substrate in the cytosolic compartment, which is included in our model [114]. Its major role is the regulation of SERCA pump activity by changing the affinity of the latter. Activation of the β₁-adrenergic signaling system leads to an increased phosphorylation of PLB by PKA, resulting in an increase in the SERCA pumping rate of Ca²⁺ from the cytosol to the SR. Dephosphorylation of PLB occurs by protein phosphatase 1 only [59], [115].

Figure 14A shows experimental and simulated time courses of PLB phosphorylation (in %) after stimulation of the β₁-adrenergic signaling system. Experimental data were obtained from rat hearts by application of 0.5 µM PKA catalytic subunit (unfilled squares, [116]) or 1 µM isoproterenol (filled circles, [117]). Data of Li et al. [118] obtained from mouse ventricular myocytes with application of 1 µM isoproterenol is shown by unfilled circles. Phosphorylation occurs rapidly, within one to two minutes of exposure to agonists. The time course is reasonably well reproduced by the model (solid line in Fig. 14A).

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Figure 14. The effects of β₁-adrenoceptor stimulation on phospholamban and troponin I.

Panel A: Experimental time courses of the phospholamban phosphorylation (in %) obtained from rat hearts [116], [117] and mouse ventricular myocytes [118]. Data Karczewski et al. [116] are obtained with application of 0.5 µM PKA catalytic subunit; data Kuschel et al. [117] and Li et al. [118] are obtained with application of 1 µM isoproterenol. Simulated time course of PLB phosphorylation is shown by a solid line. Panel B: PLB phosphorylation (in %) as functions of isoproterenol concentration. Experimental data from rat hearts [116], [117] were obtained after 2-minute exposure to isoproterenol; data from guinea pig hearts [119] were obtained after 1-minute exposure to isoproterenol; and data from rat ventricular myocytes [120] were obtained after 3-minute exposure to isoproterenol. Simulated data after 2-minute exposure to different concentrations of isoproterenol is shown by a solid line. Panel C: Experimental time courses of the troponin I phosphorylation (in %) obtained from mouse ventricular myocytes [118] after application of 1 µM isoproterenol. Simulated time course of troponin I phosphorylation is shown by a solid line. Panel D: Troponin I phosphorylation (in %) as functions of isoproterenol concentration. Experimental data from rat ventricular myocytes [120] were obtained after 3-minute exposure to isoproterenol. Simulated data after 2-minute exposure to different concentrations of isoproterenol is shown by a solid line.

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Relative phosphorylation levels of PLB after stimulation with different concentrations of isoproterenol are shown in Fig. 14B. Experimental data obtained from rat [116], [117] and guinea pig [119] hearts and from rat ventricular myocytes [120] consistently show similar half-activation isoproterenol concentration in the range from 0.003 to 0.01 µM. A similar dependence of PLB phosphorylation levels is obtained from the model after 2-minute exposure to different concentrations of isoproterenol (solid line in Fig. 14B).

Troponin I module.

Troponin I (inhibitory subunit of troponin complex) is the second substrate that is phosphorylated by PKA in the cytosolic compartment [27]. Phosphorylation of troponin I increases the Ca²⁺ unbinding rate by 50% [121], thereby decreasing the corresponding dissociation constant. Dephosphorylation of troponin I occurs by protein phosphatase 2A [61], [115].

Figure 14C shows experimental and simulated data of the time course of the relative phosphorylation level of troponin I for mouse ventricular myocytes. Experimental data were obtained by Li et al. [118] upon stimulation of cardiac cells with 1 µM isoproterenol. Both experimental and simulated data demonstrate a significant phosphorylation level of TnI without stimulation of the β₁-adrenergic signaling system. Upon application of isoproterenol, both experimental data and simulations show saturating TnI phosphorylation levels within 2 minutes of stimulation (Fig. 14C).

Dependence of the relative phosphorylation level of TnI as a function of isoproterenol concentration is shown in Fig. 14D. Both our simulations and experimental data obtained by Sulakhe and Vo [120] show a significant phosphorylation level of TnI at very low concentrations of isoproterenol. Data also demonstrates that 0.1 µM isoproterenol causes almost complete TnI phosphorylation.

Method of Simulation

The resulting model contains 141 ordinary differential equations solved by a fourth-order Runge-Kutta method, with different time steps. A relatively small time step of 0.000002 ms is used during the 10 milliseconds after the initiation of the stimulus current; the rest of the time, the time step is 0.0001 ms. Such small time steps are mainly determined by the very fast activation time constants of ryanodine receptors [25], [122]. For simulation of the cellular behavior without electrical stimulation the time step of 0.1 ms is used. The model is implemented as a program code in FORTRAN 90, which runs on a single processor under SUSE Linux 11 on a Dell Precision Workstation T3500 with six-core Intel Xeon CPU W3670 (3.2 GHz, 12 GB RAM). Simulation of one second of the activity of an electrically stimulated cell runs approximately 3 minutes on this workstation. All model equations, model parameters, and initial conditions are given in Appendix S1. The model is developed for a room temperature of 25°C (T = 298°K). Steady-state initial conditions were obtained by running the model equations without electrical stimulations until changes in each variable did not exceed 0.01%. To generate action potentials, a stimulus current, I_stim, was applied (I_stim = 80 pA/pF, τ_stim = 1 ms) with the frequencies from 1 to 5 Hz (electrical stimulation). Voltage-clamp protocols for ionic currents are described in corresponding figure legends.

Results

In this paper, our model for action potential and Ca²⁺ dynamics in an apical mouse cardiac cell [25], [26] was extended to include a β₁-adrenergic signaling system by using, in considerable part, the methodology from the previously published models [8], [10], [11], [12], [13]. Unlike models [10], [11], [12], our model represents a compartmentalized β₁-adrenergic signaling system. While the model of Hejiman et al. [8] also includes a compartmentalized β₁-adrenergic signaling system, it is developed for larger species (dog) and is verified with a different set of experimental data. In particular, our model differs from the Hejiman et al. model [8] in the following: 1) our model was verified in significant part by the experimental data from mice; 2) the model was developed for a different species (mouse) and includes a significantly different set of ionic currents; 3) the model considers non-zero phosphorylation levels of the protein kinase A substrates before activation of the β₁-adrenergic signaling system; 4) the model includes additional modulation of adenylyl cyclases by βγ-subunits of stimulatory G-protein, G_s; 5) the model data is compared in significant part with both absolute and relative magnitudes of the activities of major signaling molecules of the β₁-adrenergic signaling system; 6) the model includes two subpopulations of the L-type Ca²⁺ channels located both in the caveolae and extracaveolae compartments; 7) ryanodine receptors are localized in the extracaveolae compartment. Our model also differs from the recently published Yang and Saucerman model [12] for mouse ventricular myocytes in the following: 1) compartmentalization of β₁-adrenergic signaling system; 2) inclusion of different types of adenylyl cyclases (AC4–7) and phosphodiesterases (PDE2–4), their compartmentalization and specific regulation by drugs (e.g., rolipram, Ro 20–1724, cilostamide, milrione); 3) multicompartmental distribution of protein kinase A targets and the possibility of their separate regulation by drugs; 4) the effects of β₁-aderenergic signaling system not only on Ca²⁺ dynamics, but also on action potential.

cAMP Dynamics During Activation of β₁-adrenergic Signaling System: the Effects of Phosphodiesterases

First, we investigated the behavior of cAMP and PKA catalytic subunit concentrations in different cellular compartments in response to the activation of the β₁-adrenergic signaling system with isoproterenol. In non-stimulated cells, cAMP concentrations in caveolae, extracaveolae, and cytosol are equal to 0.2534 µM, 0.5079 µM, and 0.4078 µM, respectively. Such steady state concentrations are determined by the balance between cAMP production by adenylyl cyclases, cAMP degradation by phosphodiesterases, and cAMP fluxes between the compartments. The steady-state concentrations of cAMP were obtained by running the model equations without electrical stimulations until changes in each variable did not exceed 0.01%. The steady-state distribution of cAMP concentrations are qualitatively similar to the values obtained by Iancu et al. [13] and Heijman et al. [8]. Iancu et al. [13] data gives 0.1 µM and 1 µM of caveolar and cellular cAMP concentrations; Heijman et al. [8] data shows 0.3471 µM, 9.6236 µM, and 0.47408 µM of cAMP in the caveolae, extracaveolae, and cytosolic compartments, respectively. All simulated cellular cAMP concentrations are close to the resting cellular cAMP concentrations (∼ 0.5–1 µM) obtained experimentally [52],[53].

Figure 15A shows the simulated time courses of cAMP concentrations in different subcellular compartments in response to 1 µM isoproterenol. All cAMP transients show relatively fast rising (time-to peak is 35–70 s) and initial decaying phases due to the activation of ACs and PDEs (Fig. 15C), and relatively slow decay due to desensitization of β₁-ARs. The fastest cAMP transient is observed in the caveolae compartment because of the larger relative activities of ACs and PDEs in this compartment (see Appendix S1). In caveolae, cAMP also decays to the smaller quasi-steady-state values during desensitization of β₁-ARs. In the extracaveolae compartment, cAMP rises and decays somewhat slower than in the caveolae compartment and approaches the largest quasi-steady-state values at later times. cAMP transient in the cytosolic compartment has the largest time-to-peak value and the largest amplitude. It predominantly determines the behavior of cAMP in the cardiac cell (thick solid line). Note that the cellular cAMP concentration transient has a somewhat smaller amplitude due to its normalization to the whole cell volume V^cell.

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Figure 15. The effects of β₁-adrenoceptor stimulation on the dynamics of cAMP and PKA.

Panel A: Simulated time courses of cAMP concentrations in caveolae (thin solid line), extracaveolae (dashed line), and cytosolic compartments (dotted line), and in the whole cell volume (bold solid line) after application of 1 µM isoproterenol. Panel B: Simulated time courses of PKA catalytic subunit concentrations in caveolae (thin solid line), extracaveolae (dashed line), and cytosolic compartments (dotted line), and in the whole cell volume (bold solid line) after application of 1 µM isoproterenol. Panel C: Simulated time courses of cAMP production rate by adenylyl cyclases (solid line) and cAMP degradation rate by phosphodiesterases (dashed line) after application of 1 µM isoproterenol. Panel D: Simulated time course of cAMP fluxes between caveolae and extracaveolae (solid line), caveolae and cytosol (dashed line), and extracaveolae and cytosol (dotted line) after application of 1 µM isoproterenol. Fluxes are normalized to the cell volume V^cell.

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Figures 15C and 15D demonstrate major factors that affect cAMP transient development. cAMP increases upon relatively fast activation of adenylyl cyclases by the alpha subunit of the stimulatory G protein (G_sα) in all subcellular compartments (time-to-peak is ∼10 s). This process is accompanied by activation of phosphodiesterases, with some delay, due to the rising cAMP concentration and phosphorylation of PDEs by catalytic subunits of PKA. The interaction between ACs and PDEs reaches quasi-steady-state by ∼200 s, when their activities become close to each other. The slower part of cAMP transient is determined by the desensitization of β₁-ARs when the concentration of G_sα decreases due to its smaller production and faster re-association with G_sβγ to restore G_sαβγ. In addition to the interaction of ACs and PDEs, cAMP fluxes between the subcellular compartments contribute to cAMP transients (Fig. 15D). At early times, up to ∼30 s, the largest flux is from the caveolae to the cytosolic compartment, which is determined by the largest rising rate of cAMP in caveolae. Then this flux changes direction, and a significant amount of cAMP flows from cytosol to caveolae (dashed line in Fig. 15D). Smaller fluxes, from extracaveolae to caveolae and from cytosol to extracaveolae, are also observed during this stage of activation of β₁-ARs.

In our model, in contrast to cAMP, PKA does not move between the compartments. Its activation is determined by the type of PKA (PKAI or PKAII) and the level of cAMP in each compartment (Fig. 15B). Concentrations of catalytic subunits of PKA decay relatively slowly in extracaveolae and cytosolic compartments (dashed and dotted lines in Fig. 15B, respectively) compared to those in caveolae compartment (thin solid line in Fig. 15B), despite the relatively fast decay of cAMP concentrations in both caveolae and cytosol (Fig. 15A). Such relatively fast return of cAMP and PKA concentrations to their resting values in caveolae points to an important role of this compartment in the fast cAMP-mediated signal transduction within the β₁-adrenergic signaling system.

In addition to control conditions, we also simulated the effects of PDE3 and PDE4 inhibition on cAMP dynamics (Fig. 16). As there is no detailed experimental data on cAMP dynamics during PDE inhibition in mouse ventricular myocytes, we compared qualitatively the simulated cellular response to the data obtained for rats [123]. The data for rats shows that the selective inhibition of PDE3 by cilostamide has significantly smaller effects on cAMP transient than the selective inhibition of PDE4 by Ro 20–1724. We simulated two different methods of cAMP transient production during inhibition of PDE3 or PDE4: with continuous and pulsed application of 0.1 µM isoproterenol. Figure 16A shows that continuous application of isoproterenol from t = 0 s with simultaneous selective inhibition of PDE3 (90% inhibition) leads to an increase in peak cAMP transient by about 30%. In contrast, simultaneous application of isoproterenol and selective inhibition of PDE4 (90% inhibition) increases peak cAMP value by about ∼150%. This result points to the primary role of PDE4 in cAMP degradation compared to PDE3. Similar results were obtained experimentally in rats [123], [124]. It needs to be determined experimentally whether such predicted effect will be observed in mouse ventricular myocytes as well.

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Figure 16. The effects of PDE3 and PDE4 inhibition on cAMP dynamics upon activation of β₁-adrenergic receptors.

Panel A: Simulated time courses of cellular cAMP concentrations for control conditions (solid line), upon inhibition of PDE3 (dashed line), and upon inhibition of PDE4 (dotted line) after sustained application of 0.1 µM isoproterenol at time moment t = 0 s. Activities of PDE3 or PDE4 are inhibited by 90% to simulate the effects of corresponding selective inhibitors, cilostamide or milrione for PDE3, or rolipam or Ro 20–1724 for PDE4. Panel B: Simulated time courses of cellular cAMP concentrations for control conditions (solid line), upon inhibition of PDE3 (dashed line), and upon inhibition of PDE4 (dotted line) after pulsed application of 0.1 µM isoproterenol at time moment t = 200 s for 30 s (thick solid line). The degrees of inhibition of PDE3 and PDE4 are the same as in Panel A.

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In another set of simulations, the cells were first affected by the selective inhibitor of PDE3 (or PDE4), and then a pulse of 0.1 µM isoproterenol was applied at t = 200 s for 30 s (thick solid line in Fig. 16B). In the time interval from 0 to 200 s, the selective inhibition of PDE3 or PDE4 (both by 90%) increases steady-state cellular cAMP concentrations by ∼35% and ∼130% (Fig. 16B). Pulsed application of isoproterenol produces relatively short cAMP transients, which decay to the pre-pulse quasi-steady-state levels. When PDE3 is selectively inhibited, cAMP transient amplitude is equal to 0.6754 µM, which is ∼17% larger than the cAMP transient in control (0.5763 µM). Selective inhibition of PDE4 results in the larger cAMP transient of 0.9780 µM, or ∼69.7% larger than in control. Experimental data with pulsed application of isoproterenol and selective inhibition of PDE3 and PDE4 obtained from rat ventricular myocytes show qualitatively similar behavior [123]. Further experiments are necessary to determine whether similar effects can be observed in mice.

The Effects of Activation of the β₁-adrenergic Signaling System on Mouse Action Potential

Experimental data obtained from mouse ventricular myocytes shows that the activation of the β₁-adrenergic signaling system affects action potential shape and duration [75], [125], [126]. To simulate these effects, we stimulated the model cell with current pulses (I_stim = 80 pA/pF, τ_stim = 1.0 ms) at frequencies 1 and 5 Hz for 300 s without and with application of 1 µM isoproterenol. Figure 17A shows corresponding action potentials obtained by 1 Hz stimulation. Simulated data shows that isoproterenol prolongs mouse action potential at different degrees of repolarization. Table 1 shows the comparison of the simulated prolongations of the action potentials with the experimental data. For example, APD₅₀ and APD₉₀ are prolonged by 21.67% and 14.90%, respectively. The simulated data for APD₅₀ prolongation is close to the corresponding experimental data, 13.5±4% [126] and 18% [125] prolongation, but somewhat smaller than 48% prolongation obtained by Wang et al. [75]. In addition, the simulated data for APD₉₀ prolongation is within the experimental data variation (5±7% [126], 9% [125], and 51% [75]).

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Figure 17. Simulated action potentials and underlying ionic currents of the isolated ventricular cell model.

Simulated action potentials and underlying ionic currents are shown for control conditions and after application of 1 µM isoproterenol at two pacing frequencies 1 Hz (Panels A–E) and 5 Hz (Panels F–J) (I_stim = 80 pA/pF, τ_stim = 1.0 ms). Panels A and F: Simulated action potentials for control conditions (solid line) and after isoproterenol application (dashed line). Panels B, D, G, and I: Currents underlying the AP for control condition. Panel C, E, H, and J: Currents underlying the AP after isoproterenol application. The scales for the relatively large fast Na⁺ current, I_Na, are given on the right axis in Panels B, C, G and H. APs and ionic currents are shown after 300 s stimulation. In Panels A, C, E, F, H, and J 1 µM isoproterenol is applied at time t = 0 s.

https://doi.org/10.1371/journal.pone.0089113.g017

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Table 1. Simulated and experimental prolongations (in %) of the action potentials in mouse ventricular myocytes at different repolarizations and stimulation frequencies (1 µM Iso).

https://doi.org/10.1371/journal.pone.0089113.t001

It is remarkable that such relatively small AP prolongation due to activation of β₁-ARs is accompanied by significant changes in underlying ionic currents (Fig. 17). Simulations elucidate the mechanism of this prolongation. The four major currents are responsible for the changes in AP shape at an early stage of repolarization. The fast Na⁺ current, I_Na, changes only slightly, which leads to a small increase in AP amplitude (from 114.3 mV in control to 117.8 mV after Iso). The L-type Ca²⁺ current, I_CaL, increases almost twice upon stimulation of β₁-ARs, and promotes AP prolongation. There is also a decrease in the amplitude of the rapidly recovering transient outward K⁺ current, I_Kto,f, which also contributes to AP prolongation. An increase in the amplitude of the ultrarapidly activating K⁺ current, I_Kur, is the major opposing effect to AP prolongation, resulting in a relatively small total effect. At 90% of repolarization, four other, relatively small currents contribute to repolarization: the Na⁺/Ca²⁺ exchanger current, I_NaCa, the time-independent K⁺ current, I_K1, the Na⁺/K⁺ pump, I_NaK, and the Na⁺ background current, I_Nab. (Fig. 17, D and E). Significant increase in the magnitude of I_NaCa current upon application of isoproterenol (Fig. 17E) is one of the additional factors that cause action potential prolongation at 90% repolarization.

Simulation data obtained at stimulation frequency 5 Hz (Fig. 17, F–J) shows very similar behavior to the data for 1 Hz. The only significant change is in the peak amplitudes of the fast Na⁺ current, I_Na, which are decreased during stimulation with 5 Hz. A smaller decrease is observed for K⁺ currents I_Kto,f and I_Kur at 5-Hz stimulations. Simulation of application of 1 µM isoproterenol at 5 Hz stimulation prolongs APD₅₀ and APD₉₀ by 27.27% and 10.37%, respectively (Table 1). These prolongations are compared to the experimental data of Tong et al. [125] obtained at 4 Hz stimulation (38% and 28% prolongation for APD₅₀ and APD₉₀, respectively). Simulation data shows a correct trend of APD₅₀ prolongation, which increases with stimulation frequency. However, simulated prolongation of APD₉₀ at 5 Hz-stimulation shows somewhat smaller magnitude compared to 4 Hz-data of Tong et al. [125].

We have also simulated the effects of isoproterenol on action potential durations (APDs) at the frequencies ranged from 1 to 5 Hz. Simulation data shows relatively small increase in APDs at different levels of repolarization with stimulation frequency. For example, without isoproterenol, APD₅₀ changes from 3.0 to 3.3 ms and APD₉₀ changes from 25.5 to 27.0 ms when stimulation frequency increases from 1 to 5 Hz. Upon exposure to isoproterenol, APD₅₀ increases from 3.65 to 4.2 ms and APD₉₀ ranges from 29.3 to 30.7 ms during the same increase in stimulation frequency. Prolongation of cardiac action potential durations upon application of isoproterenol is consistently observed experimentally in mouse ventricular myocytes [75], [125], [126] (Table 1).

The Effects of Activation of the β₁-adrenergic Signaling System on Ca²⁺ Dynamics

Experimental data obtained with micromolar concentrations of isoproterenol demonstrates significant (up to 5-fold) increase in intracellular [Ca²⁺]_i transients obtained from mouse ventricular myocytes (Fig. 18, [75], [127], [128], [129]). Our simulations are able to reproduce this behavior. Figure 18, A and B, shows simulated [Ca²⁺]_i transients, obtained without and with 1 µM isoproterenol at stimulation frequencies 1 and 5 Hz. Stimulation of the β₁-adrenergic signaling system increases the simulated amplitudes of [Ca²⁺]_i at 1 Hz-stimulation from 0.44 µM to 1.92 µM (Fig. 18A), or by 4.33 fold. At larger stimulation frequency 5 Hz, [Ca²⁺]_i increases from 0.66 µM to 1.85 µM (Fig. 18B), or by 2.79 fold. These values are in good agreement with the experimental data [75], [127], [128], [129], which ranges from 2.3 to 5.2-folds increase. Frequency dependence of the diastolic and systolic [Ca²⁺]_i (Fig. 18C) demonstrates an increase of their magnitudes, with the exclusion of peak [Ca²⁺]_i at 1 µM isoproterenol and stimulation frequencies 4 and 5 Hz. It is remarkable that the model reproduces experimentally found feature such as independence of diastolic [Ca²⁺]_i from the β₁-adrenergic stimulation [128], [130].

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Figure 18. Simulated and experimental [Ca²⁺]_i transients and their characteristics in an isolated ventricular cell for control conditions and after application of isoproterenol.

Panel A: Simulated [Ca²⁺]_i transients for control conditions (solid line) and after 1 µM isoproterenol application (dashed line) obtained with 1 Hz-stimulation. Panel B: Simulated [Ca²⁺]_i transients for control conditions (solid line) and after 1 µM isoproterenol application (dashed line) obtained with 5 Hz-stimulation. Panel C: Simulated diastolic (filled symbols) and systolic (unfilled symbols) [Ca²⁺]_i magnitudes for control conditions (circles) and after 1 µM isoproterenol application (triangles) as functions of stimulation frequency. Panel D: Decay time constants for intracellular [Ca²⁺]_i transients for control conditions and after 1 µM isoproterenol application as functions of stimulation frequency. Simulated data are shown by solid (control) and dashed (1 µM isoproterenol) lines. The lines with symbols show experimental data from Benkunsky et al. [131]; experimental data from Knollmann et al. [128] are shown by squares. Panel E: Increase in [Ca²⁺]_i transient amplitudes after application of isoproterenol (folds). Model data and data of Wang et al. [75] and Liu et al. [129] are obtained at 1 Hz and 1 µM isoproterenol; data of Despa et al. [127] are obtained at 2 Hz and 1 µM isoproterenol; data of Knollmann et al. [128] are obtained at 1 Hz and 0.5 µM isoproterenol. All simulation data in this figure are obtained after 300-s stimulations and exposure to 1 µM isoproterenol.

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Our model also provides appropriate time constants for the decay of intracellular [Ca²⁺]_i and corresponding acceleration of the decay upon application of isoproterenol. Simulated and experimental frequency dependences of the decay of intracellular [Ca²⁺]_i without and with 1 µM isoproterenol are shown in Fig. 18D. The simulated time constants for the decay decrease with the stimulation frequency without and with isoproterenol and reasonably well approximate experimental data [128], [131]. Note, however, that the absolute values of [Ca²⁺]_i relaxation constants obtained by Wang et al. [75] without and with isoproterenol are significantly longer, 267 and 147 ms, respectively, but their ratio (∼1.8) is very close to the corresponding simulated value.

Our model allows for evaluation of various Ca²⁺ fluxes and their modifications by isoproterenol. Figure 19 shows simulated Ca²⁺ fluxes obtained at 1 and 5 Hz stimulations without and with 1 µM isoproterenol. Simulations show that the activation of the β₁-adrenergic signaling system leads to a significant increase in Ca²⁺ influx through the L-type Ca²⁺ channels during action potential from 1.6 µM (4.5% of released Ca²⁺ from the SR) to 3.3 µM (5.3%) at 1 Hz and from 1.8 µM (5.5%) to 3.5 µM (7.6%) at 5 Hz during cardiac cycles. Increase in Ca²⁺ influx results in an increase in the SR Ca²⁺ load, from 919 µM to 1860 µM at 1 Hz (Fig. 19E, an increase which is comparable to the experimental findings [128], [129], [132]), resulting in a growth of Ca²⁺-induced Ca²⁺ release from 36 µM to 61 µM. Smaller increase in the SR Ca²⁺ load is obtained at 5 Hz, from 1367 µM to 1602 µM, which results in an increase of Ca²⁺ release from 32 µM to 46 µM. An increase in intracellular [Ca²⁺]_i transients after application of isoproterenol also increases Ca²⁺ extrusion from the cytosol by the Na⁺/Ca²⁺ exchanger from 3.1 µM (8.6%) to 4.6 µM (7.6%) at 1 Hz and from 1.9 µM (6.0%) to 3.6 µM (7.8%) at 5 Hz; however, this increase does not completely compensate for the Ca²⁺ entry into the cell, which ultimately leads to an increase in the SR Ca²⁺ load. Only 0.18 µM and 0.28 µM (1 Hz stimulation) and 0.16 µM and 0.22 µM (5 Hz stimulation) of Ca²⁺ are extruded from the cell by a slow mechanism through the sarcolemmal Ca²⁺ pump for control conditions and after application of isoproterenol, respectively, which is about 0.5% of the released Ca²⁺ in all cases. Our model also includes background Ca²⁺ influx of ∼1.7 µM (1 Hz) and ∼0.3 µM (5 Hz) due to a very large Ca²⁺ gradient across the membrane, which does not change upon stimulation of β₁-ARs.

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Figure 19. Ca²⁺ fluxes and the SR Ca²⁺ load.

Simulated major integral Ca²⁺ fluxes during one cardiac cycle in the isolated ventricular cell model for control conditions (Panels A and C) and after application of 1 µM isoproterenol (Panels B and D). Pacing frequencies are 1 Hz (Panels A and B) and 5 Hz (Panels C and D). Major integral Ca²⁺ fluxes are shown after 300 s of stimulation. In Panels B and D 1 µM isoproterenol is applied at time t = 0 s. Here, J_CaL is the Ca²⁺ entering the cell through L-type Ca²⁺ channels; J_up – J_leak is the uptake Ca²⁺ from the cytosol to the network SR with subtracted Ca²⁺ leak from the SR to the cytosol; J_NaCa is the Ca²⁺ outflux from the cytosol through the Na⁺/Ca²⁺ exchanger; and J_pCa is the Ca²⁺ outflux through the sarcolemmal Ca²⁺ pump. Panel E: Increase in the SR Ca²⁺ load after 300-s application of isoproterenol. Model data are shown for stimulation frequencies 1, 2, 3, 4, and 5 Hz; experimental data of Liu et al. [129] and Fernandez-Velasco et al. [132] are obtained at 1 µM isoproterenol; data of Knollmann et al. [128] are obtained at 0.5 µM isoproterenol.

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Figure 20 shows the time behavior of the peak values of intracellular [Ca²⁺]_i transients and intracellular [Na⁺]_i concentration for control conditions and after application of 1 µM isoproterenol upon stimulation with frequency 1 Hz. In control, [Ca²⁺]_i transients approach quasi-steady-state values after a short-time initial decay (negative staircase effect). After application of isoproterenol, [Ca²⁺]_i transients relatively rapidly increase in amplitude during the first ∼300 seconds, and then they slowly decay. Such behavior of [Ca²⁺]_i transients is similar to the experimental data obtained by Despa et al. [127]. Initial increase in [Ca²⁺]_i transients is due to the rapid activation of β₁-adrenoceptors and cAMP accumulation; relatively slow decay of peak [Ca²⁺]_i is due to β₁-adrenoceptors desensitization. In addition, Despa et al. [127] have shown that the stimulation of β₁-ARs decreases intracellular [Na⁺]_i concentration due to an increased function of the Na⁺-K⁺ pump. Our simulation data reproduced this behavior. In control, stimulation of the model cell leads to a slight increase in [Na⁺]_i to saturating values (solid line in Fig. 20B). However, the behavior of [Na⁺]_i changes after application of isoproterenol (dashed line in Fig. 20B): after a small initial increase until peak value, [Na⁺]_i decreases subsequently in time until quasi-steady-state level. Simulated [Na⁺]_i concentration begins to decay at approximately the same time as [Ca²⁺]_i achieves its maximum value. Experimental data shows a plateau in concentration of [Na⁺]_i for a short time after application of isoproterenol, which is replaced by a decay after [Ca²⁺]_i achieves the maximum value [127].

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Figure 20. Dynamics of [Ca²⁺]_i transients and [Na⁺]_i concentrations upon stimulation of β₁-adrenoceptors.

Panel A: Simulated peak values of [Ca²⁺]_i transient as function of time for control conditions (solid line) and after 1 µM isoproterenol application at t = 0 s (dashed line). Panel B: Simulated intracellular [Na⁺]_i concentrations as function of time for control conditions (solid line) and after 1 µM isoproterenol application at t = 0 s (dashed line). In both panels, stimulation frequency is 1 Hz.

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Finally, experimental data demonstrates the absence of the negative staircase effect in [Ca²⁺]_i transients which are elicited by stimulation of a quiescent cell after application of isoproterenol [27]. The experimental data are obtained for rat ventricular myocytes, whose Ca²⁺ handling system is similar to that for mice. Our model for mouse ventricular myocytes reproduced this behavior. Figure 21A shows [Ca²⁺]_i transients upon stimulation of the quiescent cell with the frequency of 1 Hz in the control cell. The [Ca²⁺]_i decrease in time, clearly shows a negative staircase effect. In another simulation (Fig. 21B), 1 µM isoproterenol is applied to the quiescent cell for 600 seconds, and then the cell is electrically stimulated with the frequency of 1 Hz. The simulation data does not show a decrease in [Ca²⁺]_i transient amplitudes, thereby confirming the absence of a negative staircase effect after stimulation of the β₁-adrenergic signaling system.

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Figure 21. The effects of isoproterenol on negative staircase of [Ca²⁺]_i transients.

Panel A: Simulated [Ca²⁺]_i transients as function of time for control conditions show clear negative staircase effect. Panel B: Simulated [Ca²⁺]_i transients as function of time after 1 µM isoproterenol application at t = 0 s does not show negative staircase effect. In both panels, stimulation frequency is 1 Hz.

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The mechanism of two different types of behavior is explained by the analysis of the input and output Ca²⁺ fluxes without and with application of isoproterenol. Our simulations of the case without isoproterenol show that the stimulation of the quiescent myocyte increases total intracellular Ca²⁺ loss and decreases the SR Ca²⁺ load, resulting in continuous decrease in [Ca²⁺]_i transient (Fig. 21A). If the simulated cell is first pretreated with isoproterenol in the quiescent state for 600 seconds and then the electrical stimulation is applied, the Ca²⁺ fluxes inside and outside the cell remain balanced due to the predominant increase in the L-type Ca²⁺ current. The result is that the SR Ca²⁺ load is not decreased, resulting in the absence of negative staircase effect.

The Effects of Activation of the β₁-adrenergic Signaling System on Na⁺ Fluxes

Experimental data shows the effects of the β₁-adrenergic signaling system on Na⁺ dynamics in ventricular myocytes [100], [127]. In particular, in mouse ventricular myocytes, [Na⁺]_i decreases upon stimulation of β₁-adrenergic receptors. Such behavior was reproduced by our model as well (Fig. 20B). In addition, our model is able to predict major Na⁺ fluxes into and out of the mouse ventricular myocytes. Simulated Na⁺ fluxes for control conditions and after application of 1 µM isoproterenol for stimulation frequencies of 1 and 5 Hz (I_stim = 80 pA/pF, τ_stim = 1 ms) are shown in Fig. 22. Na⁺ enters the cell through the fast Na⁺ channels, Na⁺/Ca²⁺ exchanger, and background mechanisms (large Na⁺ gradient and other exchangers and co-transporters [133]), and is pumped out of the cell by the Na⁺-K⁺ pump. Without isoproterenol and at 1 Hz stimulation, 3.8 µM of Na⁺ enter the cell during action potential through the fast Na⁺ channels (6.5% of the total Na⁺ influx), 9.3 µM of Na⁺ through the Na⁺/Ca²⁺ exchanger (16%), and 45.5 µM of Na⁺ through the background mechanism (77.5%), giving total Na⁺ influx of 58.6 µM. After application of 1 µM isoproterenol and 1 Hz stimulation, the total Na⁺ influx into the cell increases to 64.0 µM, resulting in proportional changes of Na⁺ influx through the fast Na⁺ channels (4.2 µM, or 6.5%), increased influx through the Na⁺/Ca²⁺ exchanger (13.9 µM, or 22%), and unchanged Na⁺ influx through the background mechanism (45.9 µM, or 71.5%). At the larger stimulation frequency (5 Hz), the contribution of the different Na⁺ entry mechanisms changes. Without isoproterenol, 3.6 µM of Na⁺ enter the cell during action potential through the fast Na⁺ channels (20% of the total Na⁺ influx), 5.8 µM of Na⁺ through the Na⁺/Ca²⁺ exchanger (32%), and 8.9 µM of Na⁺ through the background mechanism (48%), yielding total Na⁺ influx of 18.3 µM. Application of 1 µM isoproterenol increases the total Na⁺ influx into the cell to 24.4 µM, resulting in an increase of Na⁺ influx through the fast Na⁺ channels (3.9 µM, or 17%) and the Na⁺/Ca²⁺ exchanger (10.7 µM, or 46%), and unchanged Na⁺ influx through the background mechanism (8.9 µM, or 37%).

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Figure 22. The effects of isoproterenol on integral Na⁺ fluxes.

Simulated major integral Na⁺ fluxes during one cardiac cycle in the isolated ventricular cell model are shown for control conditions (Panels A and C) and after application of 1 µM isoproterenol (Panels B and D). Pacing frequencies are 1 Hz (Panels A and B) and 5 Hz (Panels C and D). Major integral Na⁺ fluxes are shown after 300 s of stimulation. In Panels B and D 1 µM isoproterenol is applied at time t = 0 s. Here, J_Nav is the Na⁺ entering the caveolae compartment through the fast Na⁺ channels; J_Nab is the background Na⁺ influx; J_NaCa is the Na⁺ influx to the cytosol through the Na⁺/Ca²⁺ exchanger; and J_NaK is the Na⁺ outflux through the Na⁺-K⁺ pump.

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Thus, our simulations allow for the estimation of Na⁺ fluxes and dynamics, and their modifications by the β₁-adrenergic signaling system. The model data shows an increased fraction of voltage-dependent Na⁺ entry into the cell at higher stimulation frequencies and the shift of the balance of the Na⁺ fluxes upon application of isoproterenol towards outside the cell due to an increased function of the Na⁺-K⁺ pump.

The Effects of the Block of Different Populations of I_CaL on the Action Potential and [Ca²⁺]_i Transients

Experimental data shows that two different populations of the L-type Ca²⁺ channels, in caveolin-3-rich and caveolin-3-free membrane fractions, affects differently [Ca²⁺]_i transients and cellular contraction [70]. Such investigations were performed by a specific block of the caveolae-linked L-type Ca²⁺ channels. While the experiments show a 10% decrease in the mean values of the peak of [Ca²⁺]_i transients in the myocytes with blocked caveolae-located L-type Ca²⁺ channels compared to control, such decrease did not reach statistical significance. Similar small, but not significant, decrease was also observed in myocyte contraction.

We used the model to investigate the effects of the L-type Ca²⁺ channel block in different cellular compartments on the action potential and [Ca²⁺]_i transients in control and after application of 1 µM isoproterenol (Fig. 23). The model cells are electrically stimulated at the frequency 1 Hz. In control, we observed a little change in action potential shape when the caveolae-linked I_CaL (I_CaL,cav) is blocked (APD₅₀ decreased by only 2%), whereas a much larger change in the AP is observed during block of I_CaL in the extracaveolae compartment (I_CaL,ecav) (APD₅₀ decreased by 14%) (Fig. 23, A). The magnitude of the total I_CaL changed by ∼20% during the block of I_CaL,cav, while the I_CaL is almost abolished by the block of I_CaL,ecav (Fig. 23, B). The I_CaL,cav block relatively slightly (by 25%) decreases [Ca²⁺]_i transients, similar to the experimental finding by [70], while at the I_CaL,ecav block such transient is not present (Fig. 23, C).

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Figure 23. The effects of two subpopulations of the L-type Ca²⁺ current block on the action potentials and [Ca²⁺]_i transients.

Simulated effects of two subpopulations of the L-type Ca²⁺ current block on the action potentials and [Ca²⁺]_i transients in the isolated ventricular cell model are shown for control conditions and after application of 1 µM isoproterenol at pacing frequency 1 Hz (I_stim = 80 pA/pF, τ_stim = 1.0 ms). Panels A–C: Control conditions; Panels D–F: Isoproterenol is applied. Panels A and D: Simulated action potentials for control conditions (solid black line), after I_CaL,ecav block (green line), and after I_CaL,cav block (red line). Panels B and E: Simulated I_CaL currents. Panel C and F: Simulated [Ca²⁺]_i transients. APs and ionic currents are shown after 300 s stimulation. 1 µM isoproterenol is applied at time t = 0 s.

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When the model cell is stimulated by isoproterenol, the specific block of I_CaL,cav only slightly decreased the total cellular I_CaL (Fig. 23, E), resulting in more pronounced shortening of APD₅₀ (by 8%, Fig. 23, D) compared to control. Even larger AP shortening is obtained with the specific block of I_CaL,ecav (by 28%). More significant effect of I_CaL,cav block on [Ca²⁺]_i transients is predicted by simulations with isoproterenol than for control conditions (a decrease by 28%), and [Ca²⁺]_i transients is almost abolished with the I_CaL,ecav block (Fig. 23, F). Further experiments on the effects of different populations of the L-type Ca²⁺ channels on the action potential and [Ca²⁺]_i transients are necessary to verify model predictions.

Discussion

In this paper, a new compartmentalized model for the β₁-adrenergic signaling system in mouse ventricular myocytes is developed. This model is based on our previously published model for an apical cardiac cell [25], [26], which includes a comprehensive description of action potential, ionic currents, and Ca²⁺ dynamics. The new model includes biochemical and electrophysiological parts of the β₁-adrenergic signaling pathway, which are extensively verified by the existing experimental data. The model successfully reproduces cAMP dynamics, activation of adenylyl cyclases and phosphodiesterases, protein kinase A and its targets, voltage-clamp protocols for major repolarization currents, action potential modification, and changes in the Ca²⁺ handling mechanism upon stimulation of the β₁-adrenergic signaling system. The model allows for elucidation of the mechanisms of action potential prolongation and increase in [Ca²⁺]_i transients. Simulations also show the absence of the negative staircase effect in [Ca²⁺]_i transients upon stimulation of β₁-adrenoceptors, which was found experimentally. The model also allows for some testable predictions, such as frequency dependences of action potential durations and [Ca²⁺]_i transient amplitudes. The model highlights the importance of compartmentalization of the β₁-adrenergic signaling system in mouse ventricular myocytes by the description of the two populations of the L-type Ca²⁺ channels, in caveolae and extracaveolae compartments, and their distinct functional role in myocyte function, as well as the differential localization and function of other PKA targets.

Compartmentalization of the β₁-adrenergic Signaling System

The β-adrenergic signaling system plays a significant role in the function of the heart. There are two types of β-adrenergic receptors in cardiomyocytes (β₁- and β₂-adrenergic receptors), which are different in their cellular localization and function. Experimental data from rat ventricular myocytes by Rybin et al. [20] shows that β₁-adrenergic receptors are distributed between caveolae, non-caveolae membrane fractions, and internal membranes, with the majority of the β₁-adrenergic receptors being found outside of the caveolae compartment. In contrast, β₂-adrenergic receptors (β₂-ARs) are localized in the caveolae compartment [20]. Similar data were obtained for mouse ventricular myocytes [19]. According to the experimental finding, our model includes only 1% of β₁-adrenergic receptors in the caveolae compartment, with the majority of them distributed between the extracaveolae and cytosolic compartments. Such localization suggests different functional consequences: selective activation of β₁-adrenergic receptors with isoproterenol in mouse ventricular myocytes leads to a significant increase in [Ca²⁺]_i transient and myocyte contraction, while selective activation of β₂-adrenergic receptors with zinterol does not have any effect on myocyte contractility [134]. Activation of β₁-adrenergic receptors also results in phosphorylation of major cytosolic proteins, such as phospholamban and troponin I, while stimulation of β₂-adrenergic receptors does not produce this effect [135].

In addition to differential localization of β₁- and β₂-adrenergic receptors, experimental data also demonstrates differential localization of signaling proteins involved in the β₁-adrenergic signaling pathway, suggesting that even activation of one signaling system is a complex process, which proceeds differently in separate compartments. It has been found that adenylyl cyclases of type V/VI are predominantly localized in caveolae, while types IV and VII are located in non-caveolae membrane fractions and cytosol [28], [35], [36]. There is also differential distribution of three major types of phosphodiesterases in subcellular compartments (PDE2, PDE3, and PDE4 [48]), which also causes different effects on cAMP degradation [123]. Our model successfully reproduces the activities of ACs and PDEs in different compartments, and the differential effects of PDE3 and PDE4 inhibition in production of cAMP transients. For example, steady-state cAMP concentration is smaller and cAMP transient is less prolonged in the caveolae compartment than in the extracaveolae and cytosol (Fig. 15), suggesting larger activity of PDEs in the caveolae.

Finally, the major protein kinase A phosphorylation targets are also localized in different subcellular compartments. Two of them are found predominantly in the caveolae compartment (the fast Na⁺ current and the phospholemman, which regulates the Na⁺-K⁺ pump), five others (I_CaL, I_Kto,f, I_Kur, I_K1, and ryanodine receptors) are predominantly expressed in non-caveolae membrane domains, and phospholamban and troponin I are located in the cytosol (see Methods for details). It is remarkable that one of the PKA targets, the L-type Ca²⁺ channel, is expressed in both the caveolae and extracaveolae compartments, with different a physiological role in each domain. In addition to the different distribution of two major protein kinase A isoforms (PKAI and PKAII), there is also a different localization of the major dephosphorylation proteins (protein phosphatase 1 and protein phosphatase 2A). Both PP1 and PP2A are found in the caveolae and cytosolic compartments, however, only PP1 plays an important functional role in the extracaveolae. Such distribution of the targets results in their different phosphorylation kinetics and magnitude, producing a very complex interaction relationship in the effects on action potential and [Ca²⁺]_i transients.

Our model of the β₁-adrenergic signaling system includes differential subcellular localization of both signaling and target proteins, and is able to reproduce both phosphorylation kinetics and concentration-dependence of protein phosphorylation by isoproterenol (see Methods). Several non-compartmentalized models were developed for β₁-adrenergic signaling system in different species, including mice [9], [10], [11], [12]. The models were extensively verified by the available experimental data on the effects of activation of β₁-adrenergic receptors on electrical activity and ionic homeostasis. However, as the experimental technique is improving and the new data on subcellular organization of signaling systems is accumulating, more comprehensive models are required for more precise description of the cellular functions. Such important findings include differential localization of the isoforms of the major signaling proteins in the β₁-adrenergic signaling system: adenylyl cyclases, phosphodiesterases, and protein kinase A [10], [36], [46]. Discovery of the differential localization of the targets of PKA, such as the ionic currents and contractile proteins, requires more demands on the models of cardiac cells to include multiple subcellular compartments. One of the recent experimental findings of the two populations of the L-type Ca²⁺ channels, the major players in cardiac excitation-contraction coupling, and their differential physiological role in cellular function highlights the needs in compartmentalized models of cardiac myocytes [21], [22]. One such model was developed recently for canine ventricular myocytes and includes three signaling systems, β₁- and β₂-adrenergic, and CaMKII-mediated signaling systems [8]. The model described well extensive experimental data and the effects of different signaling systems on the cardiac action potential and [Ca²⁺]_i transients. Our model of the β₁-adrenergic signaling system consists of some elements of the model of Heijman et al. [8], but with significant differences, as outlined above. In particular, the presented model includes different localization of ryanodine receptors and describes two populations of the L-type Ca²⁺ channels based on the most recent experimental data [21], [22]. While the major role of compartmentalization of the components in the β₁-adrenergic signaling system is clear – separation of the effects of different signaling proteins – the particular role of the signaling molecules in the mechanisms of regulation of the target proteins still needs to be determined.

The Effects of the β₁-adrenergic Signaling System on Action Potential

Experimental data shows that the activation of the β₁-adrenergic signaling system moderately prolongs action potentials duration in mouse ventricular myocytes (Table 1, [125], [126]). Our previous simulation data using the models of mouse ventricular myocytes and ventricular tissues show that the prolongation of action potential can be a pro-arrhythmic factor causing a loss of stability at the cellular level [136] or action potential block at the tissue level at fast pacing rates [137]. Our model reproduces action potential prolongation and elucidates its mechanism. We found that the major effect on action potential at 25% and 50% repolarization comes from an increase in the inward L-type Ca²⁺ current, I_CaL, and the fast Na⁺ current, I_Na, and a decrease in the rapidly recovering transient outward K⁺ current, I_Kto,f, which tend to prolong action potential, and an increase in the ultra-rapidly activating current, I_Kur, whose role is in action potential shortening (Fig. 17). At 75% and 90% repolarization, more currents, such as the Na⁺/Ca²⁺ exchanger current, the Na⁺-K⁺ pump current, the time-independent K⁺ current, I_K1, and the Na⁺ background current, I_Nab, are brought into play (Fig. 17). The total result of interaction is the moderate prolongation of action potential duration. Note that similar prolongation of the action potential duration upon stimulation of the β₁-adrenergic signaling system was found in rat ventricular cells [10], however, the mechanism of the action potential prolongation and the role of major contributing currents were not investigated.

Frequency dependences of the action potential duration at different levels of repolarization show their different prolongations upon stimulation with isoproterenol (Table 1). While the prolongations of APD₅₀ increase with the stimulation frequency, the prolongations of APD₇₅ and APD₉₀ demonstrate more complex behavior. Such differences are explained by the different major contributing currents to AP duration at different levels of repolarization without and with isoproterenol. A decrease in the prolongation magnitude of APD₉₀ compared to APD₅₀ upon application of isoproterenol is also observed in some experiments [125], [126]; however, data of Wang et al. [75] demonstrated similar prolongations both for APD₉₀ and APD₅₀. Further experiments are necessary to investigate this phenomenon.

This effect of β₁-adrenergic receptor stimulation on action potential is different from that in larger species [8], [11]. Experimental data shows that stimulation of β₁-ARs reduces action potential duration in rabbits and dogs wild type ventricular myocytes [11], [138]. The data of Volders et al. [138] shows that one of the major contributing factors in action potential shortening is an increase in the slow delayed-rectifier current, I_Ks, upon activation of β₁-ARs. The increase in I_Ks overcomes the tendency of action potential to prolongation due to an increase in the L-type Ca²⁺ current, I_CaL [138]. This result was also confirmed by simulations using models for rabbit and canine action potential which include the β₁-adrenergic signaling system [8], [11].

Thus, our model for the β₁-adrenergic signaling system in mouse ventricular myocytes and the models of others for canine and rabbit cardiac cells [8], [11] demonstrate different effects of β₁-adrenoceptor stimulations on the action potential durations, elucidate the mechanisms of these effects, and reveal the different ionic currents which are responsible for the changes.

The Effects of the β₁-adrenergic Signaling System on Ca²⁺ Dynamics

As found experimentally, activation of the β₁-adrenergic signaling system significantly increases the magnitude of intracellular [Ca²⁺]_i transients, depending on the concentration of β₁-ARs agonist [75], [127], [128], [129], [139]. The effect is more pronounced in rodent ventricular cells where the increase can reach up to 5 times [127], and a smaller effect is observed in larger species, such as rabbit and dog [139], [140]. In addition to an increase in [Ca²⁺]_i transient amplitude, β₁-AR agonists increase the rate of [Ca²⁺]_i decline.

There are several points of view on what is the major cause of the inotropy and lusitropy in the heart. It is clear that phosphorylation of phospholamban increases the pumping of Ca²⁺ into the SR upon stimulation of β₁-AR and is considered a crucial regulator of cardiac function [27], [141]. However, this phospholamban phosphorylation is not the only reason for such increase. Recently Eisner et al. [142] analyzed the major contributing factor to positive cardiac inotropy upon stimulation of β₁-ARs. They considered four proteins that are affected by adrenergic stimulation: ryanodine receptors, SERCA pump, L-type Ca²⁺ channels, and troponin. Their analysis has shown that the L-type Ca²⁺ current is a major player that leads to positive cardiac inotropy. In our model, stimulation of the β₁-adrenergic signaling system increases I_CaL by about twice compared to control cells (Fig. 9 [79], [80], [81]). This increase approximately doubles Ca²⁺ influx into the myocyte (see also our simulation data in Fig. 19), while Ca²⁺ extrusion from the myocyte, predominantly by the Na⁺/Ca²⁺ exchanger, does not increase to the same degree. The resulting effect is an increase in Ca²⁺ influx into cell until a new dynamic quasi-steady-state is reached. Thus, our modeling data supports the view that the L-type Ca²⁺ current is a major player in cardiac inotropy in mouse ventricular myocytes, as also suggested by Eisner et al. [142].

Our model also supports the idea that the key contributor to cardiac lusitropy upon stimulation of β₁-ARs is the SERCA Ca²⁺ pump. In mouse and rat ventricular myocytes, about 90% of the released Ca²⁺ is pumped back to the sarcoplasmic reticulum compared to about 70% in rabbits and larger species [27]. An estimation of Ca²⁺ influx into the SR by the SERCA pump during one cardiac cycle (1 Hz stimulation) before and after activation of the β₁-adrenergic signaling system is 36 µM and 61 µM, respectively. This estimation correlates with about a two-fold decrease in the time constant of [Ca²⁺]_i relaxation (Fig. 18). While the Na⁺/Ca²⁺ exchanger also contributes to the [Ca²⁺]_i relaxation, its contribution in mouse ventricular myocytes is less than 10%. In larger species, the Na⁺/Ca²⁺ exchanger can make a larger contribution to the lusitropic effect, as its share is about 25–30% of the total released Ca²⁺.

There is also a long-term dispute among two groups of scientists who study ryanodine receptors (Marks group on the one hand and Valdivia and Houser group on the other) related to the physiological role of RyR phosphorylation in cardiac function [143]. Experimental data of Marks and co-authors demonstrated that enhanced phosphorylation of RyRs at S2808 in failing hearts results in an increased Ca²⁺ leak from the SR and leads to an increased arrhythmias [143], [144]. The Houser and Valdivia group have shown opposite results: they found that RyR phosphorylation site S2808 does not produce significant physiological effects neither in wild type nor in infarcted mouse hearts [145]. Our simulations shows that phosphorylation of RyRs does not change Ca²⁺ sensitivity and does not produce significant physiological effect during stimulation of the β₁-adrenergic signaling system, the results which are in line with the data from Houser and Valdivia group.

The Effects of the β₁-adrenergic Signaling System on Na⁺ Fluxes

Our model of the β₁-adrenergic signaling system in mouse ventricular myocytes is able to reproduce experimental data on a decrease in [Na⁺]_i concentration upon activation of β₁-ARs (Fig. 20, [100], [127]). We also estimated a contribution of the different mechanisms of the Na⁺ entry and extrusion from the cell, experimental data for which are not available yet. Simulations at physiological frequency 5 Hz and without application of isoproterenol suggest that about 20% of Na⁺ enter the cell through the fast Na⁺ current, 32% through the Na⁺/Ca²⁺ exchanger, and 48% through the background mechanisms (large Na⁺ gradient, the Na⁺/H⁺ exchanger, the Na⁺/HCO⁻₃ co-transporter, etc.). With application of isoproterenol, the fraction of Na⁺ entry decreases for the fast Na⁺ current to 17%, increases to 46% for the Na⁺/Ca²⁺ exchanger, and decreases to 37% for the background mechanism. These fractions are different from those estimated for the larger species, such as rabbits [133]. For rabbits, about 22% of Na⁺ enter the cell through the fast Na⁺ current (which is similar to our estimations for mice), 60% through the Na⁺/Ca²⁺ exchanger, and 18% through the background mechanisms, suggesting the Na⁺/Ca²⁺ exchanger to be the major player in the Na⁺ transport into the cell. Further experiments are necessary to verify Na⁺ fluxes structure in mouse ventricular cells without and with application of isoproterenol estimated from the presented model.

Model Limitations

Despite that the presented model was extensively verified by the experimental data and reproduced most effects which result from stimulation of the β₁-adrenergic signaling system, it has some limitations. One of these limitations is that some experimental data used for the model verification were obtained from different species, such as rats, canine, and rabbits. In this respect, some of the model parameters can be adjusted to fit the data obtained from mouse ventricular myocytes, when such data becomes available. A second source of the errors in model parameters is the low accuracy of biochemical experiments, which can vary by an order of magnitude (see for example data on PKA activation by cAMP). However, investigations by Soltis and Saucerman [146] are very encouraging about this issue. They have shown that the β₁-adrenergic signaling system is robust, at least in steady-state, even when the model parameters change by 1–2 orders of magnitude. Third, not all model parameters are measured directly in the experiments, and, therefore, are adjusted numerically to fit the experimental data downstream in the signaling pathway. Finally, a fourth limitation comes from the availability of at least two other, β₂-adrenergic and CaMKII-mediated, signaling systems that can potentially interact with the β₁-adrenergic system. Experimental data with mice shows that the β₂-adrenergic signaling system does not affect the β₁-adrenergic system in control and upon application of isoproterenol [7]. This phenomenon is explained by the significantly larger concentration of the inhibitory G protein, G_i, compared to G_s in mouse ventricular cells, which inhibits the stimulatory effects of the β₂-ARs. The effects of β₂-ARs can only be revealed upon additional application of pertussis toxin which suppresses the activity of G_i [7]. While the effects of the CaMKII-mediated signaling system are not taken into account in the presented model, the model of the β₁-adrenergic signaling system still describes reasonably well most of the available experimental data on mouse ventricular myocytes. The author considers this model as the first step in the development of a more comprehensive compartmentalized model of the adrenergic signaling system in mouse ventricular myocytes.

Supporting Information

Appendix S1.

Model equations and parameters.

https://doi.org/10.1371/journal.pone.0089113.s001

(PDF)

Acknowledgments

The author would like to thank Drs. H. Abriel, S. O. Døskeland, A. El-Armouche, J. Heijman, A. N. Lopatin, L. S. Maier, M. J. Morales, R. L. Rasmusson, and J. J. Saucerman for their valuable comments related to the different subjects of this paper, Brent Wooldridge for drawing the scheme of the β₁-adrenergic signaling system, and Paula D. Mullins for careful reading of the manuscript.

Author Contributions

Conceived and designed the experiments: VEB. Performed the experiments: VEB. Analyzed the data: VEB. Contributed reagents/materials/analysis tools: VEB. Wrote the paper: VEB.

References

1. Rudy Y, Ackerman MJ, Bers DM, Clancy CE, Houser SR, et al. (2008) System approach to understanding electromechanical activity in the human heart: a National Heart, Lung, and Blood Institute workshop summary. Circulation 118: 1202–1211.
- View Article
- Google Scholar
2. Schaub MC, Hefti MA, Zaugg M (2006) Integration of calcium with the signaling network in cardiac myocytes. J Mol Cell Cardiol 41: 183–214.
- View Article
- Google Scholar
3. Wachter SB, Gilbert EM (2012) Beta-adrenergic receptors, from their discovery and characterization through their manipulation to beneficial clinical application. Cardiology 122: 104–112.
- View Article
- Google Scholar
4. Ho D, Yan L, Iwatsubo K, Vatner DE, Vatner SF (2010) Modulation of β-adrenergic receptor signaling in heart failure and longevity: targeting adenylyl cyclase type 5. Heart Fail Rev 15: 495–512.
- View Article
- Google Scholar
5. Reincober J, Tscheschner H, Pleger ST, Most P, Katus HA, et al. (2012) Targeting GRK2 by gene therapy for heart failure: benefits above β-blockade. Gene Ther 19: 686–693.
- View Article
- Google Scholar
6. Shah AM, Mann DL (2011) In search of new therapeutic targets and strategies for heart failure: recent advances in basic science. Lancet 378: 704–712.
- View Article
- Google Scholar
7. Xiao RP, Zhu W, Zheng M, Chakir K, Bond R, et al. (2004) Subtype-specific β-adrenoceptor signaling pathways in the heart and their potential clinical implications. Trends Pharmacol Sci 25: 358–365.
- View Article
- Google Scholar
8. Heijman J, Volders PGA, Westra RL, Rudy Y (2011) Local control of β-adrenergic stimulation: effects on ventricular myocyte electrophysiology and Ca²⁺ transient. J Mol Cell Cardiol 50: 863–871.
- View Article
- Google Scholar
9. Kuzumoto M, Takeuchi A, Nakai H, Oka C, Noma A, et al. (2008) Simulation analysis of intracellular Na⁺ and Cl⁻ homeostasis during β1-adrenergic stimulation of cardiac myocytes. Prog Biophys Mol Biol 96: 171–186.
- View Article
- Google Scholar
10. Saucerman JJ, Brunton LL, Michailova AP, McCulloch AD (2003) Modeling β-adrenergic control of cardiac myocyte contractility in silico. J Biol Chem 278: 47997–48003.
- View Article
- Google Scholar
11. Saucerman JJ, Healy SN, Belik ME, Puglisi JL, McCulloch AD (2004) Proarrhythmic consequences of a KCNQ1 AKAP-binding domain mutation: computational models of whole cells and heterogeneous tissue. Circ Res 95: 1216–1224.
- View Article
- Google Scholar
12. Yang JH, Saucerman JJ (2012) Phospholemman is a negative feed-forward regulator of Ca²⁺ in β-adrenergic signaling, accelerating β-adrenergic inotropy. J Mol Cell Cardiol 52: 1048–1055.
- View Article
- Google Scholar
13. Iancu RV, Jones SW, Harvey RD (2007) Compartmentation of cAMP signaling in cardiac myocytes: a computational study. Biophys J 92: 3317–3331.
- View Article
- Google Scholar
14. Iancu RV, Ramamurthy G, Warrier S, Nikolaev VO, Lohse MJ, et al. (2008) Cytoplasmic cAMP concentrations in intact cardiac myocytes. Am J Physiol Cell Physiol 295: C414–C422.
- View Article
- Google Scholar
15. Maguy A, Hebert TE, Nattel S (2006) Involvement of lipid rafts and caveolae in cardiac ion channel function. Cardiovasc Res 69: 798–807.
- View Article
- Google Scholar
16. Balijepalli RC, Kamp TJ (2008) Caveolae, ion channels and cardiac arrhythmias. Prog Biophys Mol Biol 98: 149–160.
- View Article
- Google Scholar
17. Harvey RD, Calaghan SC (2012) Caveolae create local signalling domains through their distinct protein content, lipid profile and morphology. J Mol Cell Cardiol 52: 366–375.
- View Article
- Google Scholar
18. Weiss S, Oz S, Benmocha A, Dascal N (2013) Regulation of cardiac L-type Ca²⁺ channel Ca_V1.2 via the β-adrenergic-cAMP-protein kinase A pathway. Old dogmas, advances, and new uncertainties. Circ Res 113: 617–631.
- View Article
- Google Scholar
19. Balijepalli RC, Foell JD, Hall DD, Hell JW, Kamp TJ (2006) Localization of cardiac L-type Ca²⁺ channels to a caveolar macromolecular signaling complex is required for β₂-adrenergic regulation. Proc Natl Acad Sci USA 103: 7500–7505.
- View Article
- Google Scholar
20. Rybin VO, Xu X, Lisanti MP, Steinberg SF (2000) Differential targeting of β-adrenergic receptor subtypes and adenylyl cyclase to cardiomyocyte caveolae: a mechanism to functionally regulate the cAMP signaling pathway. J Biol Chem 275: 41447–41457.
- View Article
- Google Scholar
21. Scriven DRL, Asghari P, Schulson MN, Moore EDW (2010) Analysis of Ca_V1.2 and ryanodine receptor clusters in rat ventricular myocytes. Biophys J 99: 3923–3929.
- View Article
- Google Scholar
22. Best JM, Kamp TJ (2012) Different subcellular populations of L-type Ca²⁺ channels exhibit unique regulation and functional roles in cardiomyocytes. J Mol Cell Cardiol 52: 376–387.
- View Article
- Google Scholar
23. Engelhardt S, Hein L, Wiesmann F, Lohse MJ (1999) Progressive hypertrophy and heart failure in β₁-adrenergic receptor transgenic mice. Proc Natl Acad Sci USA 96: 7059–7064.
- View Article
- Google Scholar
24. Milano CA, Allen LF, Rockman HA, Dolber PC, McMinn TR, et al. (1994) Enhanced myocardial function in transgenic mice overexpressing the β₂-adrenergic receptor. Science 264: 582–586.
- View Article
- Google Scholar
25. Bondarenko VE, Szigeti GP, Bett GCL, Kim SJ, Rasmusson RL (2004) Computer model of action potential; of mouse ventricular myocytes. Am J Physiol Heart Circ Physiol 287: H1378–H1403.
- View Article
- Google Scholar
26. Petkova-Kirova PS, London B, Salama G, Rasmusson RL, Bondarenko VE (2012) Mathematical modeling mechanisms of arrhythmias in transgenic mouse heart overexpressing TNF-α. Am J Physiol Heart Circ Physiol 302: H934–H952.
- View Article
- Google Scholar
27. Bers DM (2001) Excitation-Contraction Coupling and Cardiac Contractile Force (2^nd ed.). Dordrecht, The Netherlands: Kluwer Academic. 427 p.
28. Steinberg SF (2004) β₂-adrenergic receptor signaling complexes in cardiomyocyte caveolae/lipid rafts. J Mol Cell Cardiol 37: 407–415.
- View Article
- Google Scholar
29. Hilal-Dandan R, Kanter JR, Brunton LL (2000) Characterization of G-protein signaling in ventricular myocytes from the adult mouse heart: differences from the rat. J Mol Cell Cardiol 32: 1211–1221.
- View Article
- Google Scholar
30. Nikolaev VO, Moshkov A, Lyon AR, Miragoli M, Noval P, et al. (2010) β₂-adrenergic receptor redistribution in heart failure changes cAMP compartmentation. Science 327: 1653–1657.
- View Article
- Google Scholar
31. Lohse MJ, Hein P, Hoffmann C, Nikolaev VO, Vilardaga JP, et al. (2008) Kinetics of G-protein-coupled receptor signals in intact cells. Br J Pharmacol 153: S125–S132.
- View Article
- Google Scholar
32. Freedman NJ, Liggett SB, Drachman DE, Pei G, Caron MG, et al. (1995) Phosphorylation and desensitization of the human β₁-adrenergic receptor: involvement of G protein-coupled receptor kinases and cAMP-dependent protein kinase. J Biol Chem 270: 17953–17961.
- View Article
- Google Scholar
33. Göttle M, Geduhn J, König B, Gille A, Höcherl K, et al. (2009) Characterization of mouse heart adenylyl cyclase. J Pharmacol Exp Ther 329: 1156–1165.
- View Article
- Google Scholar
34. Tang T, Gao MH, Lai NC, Firth AL, Takahashi T, et al. (2008) Adenylyl cyclase type 6 deletion decreases left ventricular function via impaired calcium handling. Circulation 117: 61–69.
- View Article
- Google Scholar
35. Head BP, Patel HH, Roth DM, Lai NC, Niesman IR, et al. (2005) G-protein-coupled receptor signaling components localize in both sarcolemmal and intracellular caveolin-3-associated microdomains in adult cardiac myocytes. J Biol Chem 280: 31036–31044.
- View Article
- Google Scholar
36. Ostrom RS, Insel PA (2004) The evolving role of lipid rafts and caveolae in G protein-coupled receptor signaling: implications for molecular pharmacology. Br J Pharmacol 143: 235–245.
- View Article
- Google Scholar
37. Chen-Goodspeed M, Lukan AN, Dessauer CW (2005) Modeling of Gα_s and Gα_i regulation of human type V and VI adenylyl cyclase. J Biol Chem 280: 1808–1816.
- View Article
- Google Scholar
38. Gao B, Gilman AG (1991) Cloning and expression of a widely distributed (type IV) adenylyl cyclase. Proc Natl Acad Sci USA 88: 10178–10182.
- View Article
- Google Scholar
39. Gao X, Sadana R, Dessauer CW, Patel TB (2007) Conditional stimulation of type V and VI adenylyl cyclases by G protein βγ subunits. J Biol Chem 282: 294–302.
- View Article
- Google Scholar
40. Zimmermann G, Taussig R (1996) Protein kinase C alters the responsiveness of adenylyl cyclases to G protein α and βγ subunits. J Biol Chem 271: 27161–27166.
- View Article
- Google Scholar
41. Post SR, Hilal-Dandan R, Urasawa K, Brunton LL, Insel PA (1995) Quantification of signaling components and amplification in the β-adrenergic-receptor-adenylyl cyclase pathway in isolated adult rat ventricular myocytes. Biochem J 311: 75–80.
- View Article
- Google Scholar
42. Tepe NM, Liggett SB (1999) Transgenic replacement of type V adenylyl cyclase identifies a critical mechanism of β-adrenergic receptor dysfunction in the G_αq overexpressing mouse. FEBS Lett 458: 236–240.
- View Article
- Google Scholar
43. Lemire I, Allen BG, Rindt H, Hebert TE (1998) Cardiac-specific overexpression of α_1BAR regulates βAR activity via molecular crosstalk. J Mol Cell Cardiol 30: 1827–1839.
- View Article
- Google Scholar
44. Richter W, Xie M, Scheitrum C, Krall J, Movsesian MA, et al. (2011) Conserved expression and functions of PDE4 in rodent and human heart. Basic Res Cardiol 106: 249–262.
- View Article
- Google Scholar
45. Bode DC, Kanter JR, Brunton LL (1991) Cellular distribution of phosphodiesterase isoforms in rat cardiac tissue. Circ Res 68: 1070–1079.
- View Article
- Google Scholar
46. Fischmeister R, Castro LRV, Abi-Gerges A, Rochais F, Jurevičius J, et al. (2006) Compartmentation of cyclic nucleotide signaling in the heart: the role of cyclic nucleotide phosphodiesterases. Circ Res 99: 816–828.
- View Article
- Google Scholar
47. Osadchii OE (2007) Myocardial phosphodiesterases and regulation of cardiac contractility in health and cardiac disease. Cardiovasc Drugs Ther 21: 171–194.
- View Article
- Google Scholar
48. Mongillo M, Tocchetti CG, Terrin A, Lissandron V, Cheung YF, et al. (2006) Compartmentalized phosphodiesterase-2 activity blunts β-adrenergic cardiac inotropy via an NO/cGMP-dependent pathway. Circ Res 98: 226–234.
- View Article
- Google Scholar
49. Georget M, Mateo P, Vandecasteele G, Lipskaia L, Defer N, et al. (2003) Cyclic AMP compartmentation due to increase cAMP-phosphodiesterase activity in transgenic mice with a cardiac-directed expression of the human adenylyl cyclase type 8 (AC8). FASEB J 17: 1380–1391.
- View Article
- Google Scholar
50. Adams SR, Harootunian AT, Buechler YJ, Taylor SS, Tsien RY (1991) Fluorescence ratio imaging of cyclic AMP in single cell. Nature 349: 694–697.
- View Article
- Google Scholar
51. Dostmann WRG, Taylor SS (1991) Identifying the molecular switches that determine whether (R_p)-cAMPS functions as an antagonist or an agonist in the activation of cAMP-dependent protein kinase I. Biochemistry. 30: 8710–8716.
- View Article
- Google Scholar
52. Lin F, Owens A, Chen S, Stevens ME, Kesteven S, et al. (2001) Targeted α_1A-adrenergic receptor overexpression induces enhanced cardiac contractility but not hypertrophy. Circ Res 89: 343–350.
- View Article
- Google Scholar
53. Roman BB, Goldspink PH, Spaite E, Urboniene D, McKinney R, et al. (2004) Inhibition of PKC phosphorylation of TnI improves cardiac performance in vivo. Am J Physiol Heart Circ Physiol 286: H2089–H2095.
- View Article
- Google Scholar
54. Beavo JA, Bechtel PJ, Krebs EG (1974) Activation of protein kinase by physiological concentrations of cyclic AMP. Proc Natl Acad Sci USA 71: 3580–3583.
- View Article
- Google Scholar
55. Dao KK, Teigen K, Kopperud R, Hodneland E, Schwede F, et al. (2006) Epac1 and cAMP-dependent protein kinase holoenzyme have similar cAMP affinity, but their cAMP domains have distinct structural features and cyclic nucleotide recognition. J Biol Chem 281: 21500–21511.
- View Article
- Google Scholar
56. Hofmann F, Beavo JA, Bechtel PJ, Krebs EG (1975) Comparison of adenosine 3′: 5′-monophosphate-dependent protein kinase from rabbit skeletal and bovine heart muscle. J Biol Chem 250: 7795–7801.
- View Article
- Google Scholar
57. Buxton ILO, Brunton LL (1983) Compartments of cyclic AMP and protein kinase in mammalian cardiomyocytes. J Biol Chem 258: 10233–10239.
- View Article
- Google Scholar
58. Hescheler J, Kameyama M, Trautwein W, Mieskes G, Söling HD (1987) Regulation of the cardiac calcium channel by protein phosphatases. Eur J Biochem 165: 261–266.
- View Article
- Google Scholar
59. MacDougall LK, Jones LR, Cohen P (1991) Identification of the major protein phosphatases in mammalian cardiac muscle which dephosphorylate phospholamban. Eur J Biochem 196: 725–734.
- View Article
- Google Scholar
60. Neumann J, Boknik P, Herzig S, Schmitz W, Scholz H, et al. (1993) Evidence for physiological functions of protein phosphatases in the heart: evaluation with okadaic acid. Am J Physiol Heart Circ Physiol 265: H257–H266.
- View Article
- Google Scholar
61. duBell WH, Gigena MS, Guatimosim S, Long X, Lederer WJ, et al. (2002) Effects of PP1/PP2A inhibitor calyculin A on the E-C coupling cascade in murine ventricular myocytes. Am J Physiol Heart Circ Physiol 282: H38–H48.
- View Article
- Google Scholar
62. Müller FU, Lewin G, Baba HA, Boknik P, Fabritz L, et al. (2005) Heart-directed expression of a human cardiac isoform of cAMP-response element modulator in transgenic mice. J Biol Chem 280: 6906–6914.
- View Article
- Google Scholar
63. Herzig S, Neumann J (2000) Effects of serine/threonine protein phosphatases on ion channels in excitable membranes. Physiol Rev 80: 173–210.
- View Article
- Google Scholar
64. Carr AN, Schmidt AG, Suzuki Y, del Monte F, Sato Y, et al. (2002) Type 1 phosphatase, a negative regulator of cardiac function. Mol Cell Biol 22: 4124–4135.
- View Article
- Google Scholar
65. El-Armouche A, Wittköpper K, Degenhardt F, Weinberger F, Didié M, et al. (2008) Phosphatase inhibitor-1-deficient mice are protected from catecholamine-induced arrhythmias and myocardial hypertrophy. Cardiovasc Res 80: 396–406.
- View Article
- Google Scholar
66. Nicolaou P, Hajjar RJ, Kranias EG (2009) Role of protein phosphatase-1 inhibitor-1 in cardiac physiology and pathophysiology. J Mol Cell Cardiol 47: 365–371.
- View Article
- Google Scholar
67. Neumann J, Gupta RC, Schmitz W, Scholz H, Nairn AC, et al. (1991) Evidence for isoproterenol-induced phosphorylation of phosphatase inhibitor-1 in the intact heart. Circ Res 69: 1450–1457.
- View Article
- Google Scholar
68. O’Connell TD, Ni YG, Lin KM, Han H, Yan Z (2003) Isolation and culture of adult mouse cardiac myocytes for signaling studies. AfCS Research Reports 1: CM0005.
- View Article
- Google Scholar
69. Shibata EF, Brown TLY, Washburn ZW, Bai J, Revak TJ, et al. (2006) Autonomic regulation of voltage-gated cardiac ion channels. J Cardiovasc Electrophysiol (Suppl 1): S34–S42.
70. Makarewich CA, Correll RN, Gao H, Zhang H, Yang B, et al. (2012) A caveolae-targeted L-type Ca²⁺ channel antagonist inhibits hypertrophic signaling without reducing cardiac contractility. Circ Res 110: 669–674.
- View Article
- Google Scholar
71. Chu G, Luo W, Slack JP, Tilgmann C, Sweet WE, et al. (1996) Compensatory mechanisms associated with the hyperdynamic function of phospholamban-deficient mouse hearts. Circ Res 79: 1064–1076.
- View Article
- Google Scholar
72. Bers DM, Stiffel VM (1993) Ratio of ryanodine to dihydropyridine receptors in cardiac and skeletal muscle and implications for E-C coupling. Am J Physiol Cell Physiol 264: C1587–C1593.
- View Article
- Google Scholar
73. Bracken N, ElKadri M, Hart G, Hussain M (2006) The role of constitutive PKA-mediated phosphorylation in the regulation of basal I_Ca in isolated rat cardiac myocytes. Br J Pharmacol 148: 1108–1115.
- View Article
- Google Scholar
74. Tang M, Zhang X, Li Y, Guan Y, Ai X, et al. (2010) Enhanced basal contractility but reduced excitation-contraction coupling efficiency and β-adrenergic reserve of hearts with increased Cav1.2 activity. Am J Physiol Heart Circ Physiol 299: H519–H528.
- View Article
- Google Scholar
75. Wang H, Kohr MJ, Wheeler DG, Ziolo MT (2008) Endothelial nitric oxide synthase decreases β-adrenergic responsiveness via inhibition of the L-type Ca²⁺ current. Am J Physiol Heart Circ Physiol 294: H1473–H1480.
- View Article
- Google Scholar
76. Tsien RW, Bean BP, Hess P, Lansman JB, Nilius B, et al. (1986) Mechanisms of calcium channel modulation by β-adrenergic agents and dihydropyridine calcium agonists. J Mol Cell Cardiol 18: 691–710.
- View Article
- Google Scholar
77. Hulme JT, Westenbroek RE, Scheuer T, Catterall WA (2006) Phosphorylation of serine 1928 in the distal C-terminal domain of cardiac Ca_v1.2 channels during β1-adrenergic regulation. Proc Natl Acad Sci USA 103: 16574–16579.
- View Article
- Google Scholar
78. Kameyama M, Hescheler J, Hofmann F, Trautwein W (1986) Modulation of Ca current during the phosphorylation cycle in the guinea pig heart. Pflügers Arch 407: 123–128.
- View Article
- Google Scholar
79. Kim SJ, Yatani A, Vatner DE, Yamamoto S, Ishikawa Y, et al. (1999) Differential regulation of inotropy and lusitropy in overexpressed Gsα myocytes through cAMP and Ca²⁺ channel pathways. J Clin Invest 103: 1089–1097.
- View Article
- Google Scholar
80. Sako H, Green SA, Kranias EG, Yatani A (1997) Modulation of cardiac Ca²⁺ channels by isoproterenol studied in transgenic mice with altered SR Ca²⁺ content. Am J Physiol Cell Physiol 273: C1666–C1672.
- View Article
- Google Scholar
81. Mitarai S, Reed TD, Yatani A (2000) Changes in ionic currents and β-adrenergic receptor signaling in hypertrophied myocytes overexpressing Gα_q. Am J Physiol Heart Circ Physiol 279: H139–H148.
- View Article
- Google Scholar
82. Yarbrough TL, Lu T, Lee HC, Shibata EF (2002) Localization of cardiac sodium channels in caveolin-rich membrane domains. Regulation of sodium current amplitude. Circ Res 90: 443–449.
- View Article
- Google Scholar
83. Palygin OA, Pettus JM, Shibata EF (2008) Regulation of caveolar cardiac sodium current by a single G_sα histidine residue. Am J Physiol Heart Circ Physiol 294: H1693–H1699.
- View Article
- Google Scholar
84. Kirstein M, Eickhorn R, Kochsiek K, Langenfeld H (1996) Dose-dependent alteration of rat cardiac sodium current by isoproterenol: results from direct measurements on multicellular preparations. Pflügers Arch 431: 395–401.
- View Article
- Google Scholar
85. Matsuda JJ, Lee HC, Shibata EF (1993) Acetylcholine reversal of isoproterenol-stimulated sodium currents in rabbit ventricular myocytes. Circ Res 72: 517–525.
- View Article
- Google Scholar
86. Baba S, Dun W, Boyden PA (2004) Can PKA activators rescue Na⁺ channel function in epicardial border zone cells that survive in the infarcted canine heart? Cardiovasc Res 64: 260–267.
- View Article
- Google Scholar
87. Ono K, Fozzard HA, Hanck DA (1993) Mechanism of cAMP-dependent modulation of cardiac sodium channel current kinetics. Circ Res 72: 807–815.
- View Article
- Google Scholar
88. Zhou J, Yi J, Hu NN, George AL Jr, Murray KT (2000) Activation of protein kinase A modulates trafficking of the human cardiac sodium channel in Xenopus oocytes. Circ Res 87: 33–38.
- View Article
- Google Scholar
89. Rook MB, Evers MM, Vos MA, Bierhuizen MFA (2012) Biology of cardiac sodium channel Na_v1.5 expression. Cardiovasc Res 93: 12–23.
- View Article
- Google Scholar
90. Clancy CE, Rudy Y (2002) Na⁺ channel mutation that causes both Brugada and long-QT syndrome phenotypes: a simulation study of mechanism. Circulation 105: 1208–1213.
- View Article
- Google Scholar
91. Jayasinghe ID, Cannell MB, Soeller C (2009) Organization of ryanodine receptors, transverse tubules, and sodium-calcium exchanger in rat myocytes. Biophys J 97: 2664–2673.
- View Article
- Google Scholar
92. Wong J, Baddeley D, Bushong EA, Yu Z, Ellisman MH, et al. (2013) Nanoscale distribution of ryanodine receptors and caveolin-3 in mouse ventricular myocytes: Dilation of t-tubules near junctions. Biophys J 104: L22–L24.
- View Article
- Google Scholar
93. Xiao B, Tian X, Xie W, Jones PP, Cai S, et al. (2007) Functional consequence of protein kinase A-dependent phosphorylation of the cardiac ryanodine receptor: sensitization of store overload-induced Ca²⁺ release. J Biol Chem 282: 30256–30264.
- View Article
- Google Scholar
94. Xiao B, Zhong G, Obayashi M, Yang D, Chen K, et al. (2006) Ser-2030, but not Ser-2808, is the major phosphorylation site in cardiac ryanodine receptors responding to protein kinase A activation upon β-adrenergic stimulation in normal and failing hearts. Biochem J 396: 7–16.
- View Article
- Google Scholar
95. Takasago T, Imagawa T, Furukawa KI, Ogurusu T, Shigekawa M (1991) Regulation of the cardiac ryanodine receptor by protein kinase-dependent phosphorylation. J Biochem 109: 163–170.
- View Article
- Google Scholar
96. Xiao J, Tian X, Jones PP, Bolstad J, Kong H, et al. (2007) Removal of FKBP12.6 does not alter the conductance and activation of the cardiac ryanodine receptor or the susceptibility to stress-induced ventricular arrhythmias. J Biol Chem 282: 34828–34838.
- View Article
- Google Scholar
97. Liu L, Askari A (2006) β-Subunit of cardiac Na⁺-K⁺-ATPase dictates the concentration of the functional enzyme in caveolae. Am J Physiol Cell Physiol 291: C569–C578.
- View Article
- Google Scholar
98. Fuller W, Eaton P, Medina RA, Bell J, Shattock MJ (2001) Differential centrifugation separates cardiac sarcolemmal and endosomal membranes from Langendorff-perfused rat hearts. Anal Biochem 293: 216–223.
- View Article
- Google Scholar
99. Fuller W, Tulloch LB, Shattock MJ, Calaghan SC, Howie J, et al. (2013) Regulation of the cardiac sodium pump. Cell Mol Life Sci 70: 1357–1380.
- View Article
- Google Scholar
100. Despa S, Bossuyt J, Han F, Ginsburg KS, Jia LG, et al. (2005) Phospholemman-phosphorylation mediates the β-adrenergic effects on Na/K pump function in cardiac myocytes. Circ Res 97: 252–259.
- View Article
- Google Scholar
101. Gao J, Mathias RT, Cohen IS, Baldo GJ (1992) Isoprenaline, Ca²⁺ and the Na⁺-K⁺ pump in guinea-pig ventricular myocytes. J Physiol 449: 689–704.
- View Article
- Google Scholar
102. Abi-Char J, Maguy A, Coulombe A, Balse E, Ratajczak P, et al. (2007) Membrane cholesterol modulates Kv1.5 potassium channel distribution and function in rat cardiomyocytes. J Physiol 582: 1205–1217.
- View Article
- Google Scholar
103. Ravens U, Wettwer E (2011) Ultra-rapid delayed rectifier channels: molecular basis and therapeutic implications. Cardiovasc Res 89: 776–785.
- View Article
- Google Scholar
104. Folco EJ, Liu GX, Koren G (2004) Caveolin-3 and SAP97 form a scaffolding protein complex that regulates the voltage-gated potassium channel Kv1.5. Am J Physiol Heart Circ Physiol 287: H681–H690.
- View Article
- Google Scholar
105. Martens JR, Sakamoto N, Sullivan SA, Grobaski TD, Tamkun MM (2001) Isoform-specific localization of voltage-gated K⁺ channels to distinct lipid raft populations: targeting of Kv1.5 to caveolae. J Biol Chem 276: 8409–8414.
- View Article
- Google Scholar
106. Martínez-Mármol R, Villalonga N, Solé L, Vicente R, Tamkun MM, et al. (2008) Multiple Kv1.5 targeting to membrane surface microdomains. J Cell Physiol 217: 667–673.
- View Article
- Google Scholar
107. Li GR, Feng J, Wang Z, Fermini B, Nattel S (1996) Adrenergic modulation of ultrarapid delayed rectifier K⁺ current in human atrial myocytes. Circ Res 78: 903–915.
- View Article
- Google Scholar
108. Yue L, Feng J, Wang Z, Nattel S (1999) Adrenergic control of the ultrarapid delayed rectifier current in canine atrial myocytes. J Physiol 516: 385–398.
- View Article
- Google Scholar
109. González de la Fuente M, Barana A, Gόmez R, Amorόs I, Dolz-Gaitόn P, et al. (2013) Chronic atrial fibrillation up-regulates β1-adrenoceptors affecting repolarizing currents and action potential duration. Cardiovasc Res 97: 379–388.
- View Article
- Google Scholar
110. Hoffman DA, Johnson D (1998) Downregulation of transient K⁺ channels in dendrites of hippocampal CA1 pyramidal neurons by activation of PKA and PKC. J Neurosci 18: 3521–3528.
- View Article
- Google Scholar
111. Zhang M, Fei XW, He YL, Yang G, Mei YA (2009) Bradykinin inhibits the transient outward K⁺ current in mouse Schwann cells via the cAMP/PKA pathway. Am J Physiol Cell Physiol 296: C1364–C1372.
- View Article
- Google Scholar
112. Anumonwo JMB, Lopatin AN (2010) Cardiac strong inward rectifier potassium channels. J Mol Cell Cardiol 48: 45–54.
- View Article
- Google Scholar
113. Vaidyanathan R, Taffet SM, Vikstrom KL, Anumonwo JMB (2010) Regulation of cardiac inward rectifier potassium current (I_K1) by synapse-associated protein-97. J Biol Chem 285: 28000–28009.
- View Article
- Google Scholar
114. Simmerman HKB, Jones LR (1998) Phospholamban: protein structure, mechanism of action, and role in cardiac function. Physiol Rev 78: 921–947.
- View Article
- Google Scholar
115. Wolska BM (2009) Calcineurin and cardiac function: is more or less better for the heart? Am J Physiol Heart Circ Physiol 297: H1576–H1577.
- View Article
- Google Scholar
116. Karczewski P, Bartel S, Krause EG (1990) Differential sensitivity to isoprenaline of troponin I and phospholamban phosphorylation in isolated rat hearts. Biochem J 266: 115–122.
- View Article
- Google Scholar
117. Kuschel M, Karczewski P, Hempel P, Schlegel WP, Krause EG, et al. (1999) Ser¹⁶ prevails over Thr¹⁷ phospholamban phosphorylation in the β-adrenergic regulation of cardiac relaxation. Am J Physiol Heart Circ Physiol 276: H1625–H1633.
- View Article
- Google Scholar
118. Li L, Desantiago J, Chu G, Kranias EG, Bers DM (2000) Phosphorylation of phospholamban and troponin I in β-adrenergic-induced acceleration of cardiac relaxation. Am J Physiol Heart Circ Physiol 278: H769–H779.
- View Article
- Google Scholar
119. Lindemann JP, Jones LR, Hathaway DR, Henry BG, Watanabe AM (1983) β-adrenergic stimulation of phospholamban phosphorylation and Ca²⁺-ATPase activity in guinea pig ventricles. J Biol Chem 258: 464–471.
- View Article
- Google Scholar
120. Sulakhe PV, Vo XT (1995) Regulation of phospholamban and troponin-I phosphorylation in the intact rat cardiomyocytes by adrenergic and cholinergic stimuli: roles of cyclic nucleotides, calcium, protein kinases and phosphatases and depolarization. Mol Cell Biochem 149/150: 103–126.
- View Article
- Google Scholar
121. Robertson SP, Johnson JD, Holroyde MJ, Kranias EG, Potter JD, et al. (1982) The effect of troponin I phosphorylation on the Ca²⁺-binding properties of the Ca²⁺-regulatory site of bovine cardiac troponin. J Biol Chem 257: 260–263.
- View Article
- Google Scholar
122. Bondarenko VE, Bett GCL, Rasmusson RL (2004) A model of graded calcium release and L-type Ca²⁺ channel inactivation in cardiac muscle. Am J Physiol Heart Circ Physiol 286: H1154–H1169.
- View Article
- Google Scholar
123. Leroy J, Abi-Gerges A, Nikolaev VO, Richter W, Lechêne P, et al. (2008) Spatiotemporal dynamics of β-adrenergic cAMP signals and L-type Ca²⁺ channel regulation in adult rat ventricular myocytes: role of phosphodiesterases. Circ Res 102: 1091–1100.
- View Article
- Google Scholar
124. Mongillo M, McSorley T, Evellin S, Sood A, Lissandron V, et al. (2004) Fluorescence resonance energy transfer-based analysis of cAMP dynamics in live neonatal rat cardiac myocytes reveals distinct functions of compartmentalized phosphodiesterases. Circ Res 95: 67–75.
- View Article
- Google Scholar
125. Tong XY, Porter LM, Liu GX, Dhar-Chowdhury P, Srivastava S, et al. (2006) Consequences of cardiac myocyte-specific ablation of K_ATP channels in transgenic mice expressing dominant negative Kir6 subunits. Am J Physiol Heart Circ Physiol 291: H543–H551.
- View Article
- Google Scholar
126. Wu Y, Temple J, Zhang R, Dzhura I, Zhang W, et al. (2002) Calmodulin kinase II and arrhythmias in a mouse model of cardiac hypertrophy. Circulation 106: 1288–1293.
- View Article
- Google Scholar
127. Despa S, Tucker AL, Bers DM (2008) Phospholemman-mediated activation of Na/K-ATPase limits [Na]_i and inotropic state during β-adrenergic stimulation in mouse ventricular myocytes. Circulation 117: 1849–1855.
- View Article
- Google Scholar
128. Knollmann BC, Kirchhof P, Sirenko SG, Degen H, Greene AE, et al. (2003) Familial hypertrophic cardiomyopathy-linked mutant troponin T causes stress-induced ventricular tachycardia and Ca²⁺-dependent action potential remodeling. Circ Res 92: 428–436.
- View Article
- Google Scholar
129. Liu N, Denegri M, Ruan Y, Avelino-Cruz JE, Perissi A, et al. (2011) Short communication: Flecainide exerts an antiarrhythmic effect in a mouse model of catecholaminergic polymorphic ventricular tachycardia by increasing the threshold for triggered activity. Circ Res 109: 291–295.
- View Article
- Google Scholar
130. Song J, Gao E, Wang JF, Zhang XQ, Chan TO, et al. (2012) Constitutive overexpression of phosphomimetic phospholemman S68E mutant results in arrhythmias, early mortality, and heart failure: potential involvement of Na⁺/Ca²⁺ exchanger. Am J Physiol Heart Circ Physiol 302: H770–H781.
- View Article
- Google Scholar
131. Benkusky NA, Weber CS, Scherman JA, Farrell EF, Hacker TA, et al. (2007) Intact β-adrenergic response and unmodified progression toward heart failure in mice with genetic ablation of a major protein kinase A phosphorylation site in the cardiac ryanodine receptor. Circ Res 101: 819–829.
- View Article
- Google Scholar
132. Fernández-Velasco M, Rueda A, Rizzi N, Benitah JP, Colombi B, et al. (2009) Increased Ca²⁺ sensitivity of the ryanodine receptor mutant RyR2^R4496C underlies catecholaminergic polymorphic ventricular tachycardia. Circ Res 104: 201–209.
- View Article
- Google Scholar
133. Despa S, Bers DM (2013) Na⁺ transport in the normal and failing heart – Remember the balance. J Mol Cell Cardiol 61: 2–10.
- View Article
- Google Scholar
134. Xiao RP, Avdonin P, Zhou YY, Cheng H, Akhter SA, et al. (1999) Coupling of β₂-adrenoceptor to G_i proteins and its physiological relevance in murine cardiac myocytes. Circ Res 84: 43–52.
- View Article
- Google Scholar
135. Bers DM (2002) Cardiac excitation-contraction coupling. Nature 415: 198–205.
- View Article
- Google Scholar
136. Bondarenko VE, Rasmusson RL (2010) Transmural heterogeneity of repolarization and Ca²⁺ handling in a model of mouse ventricular tissue. Am J Physiol Heart Circ Physiol 299: H454–H469.
- View Article
- Google Scholar
137. Bondarenko VE, Rasmusson RL (2007) Simulations of propagated mouse ventricular action potentials: effects of molecular heterogeneity. Am J Physiol Heart Circ Physiol 293: H1816–H1832.
- View Article
- Google Scholar
138. Volders PGA, Stengl M, van Opstal JM, Gerlach U, Spätjens RLHMG, et al. (2003) Probing the contribution of I_Ks to canine ventricular repolarization: key role for β-adrenergic receptor stimulation. Circulation 107: 2753–2760.
- View Article
- Google Scholar
139. Pogwizd SM, Schlotthauer K, Li L, Yuan W, Bers DM (2001) Arrhythmogenesis and contractile dysfunction in heart failure: roles of sodium-calcium exchange, inward rectifier potassium current, and residual β-adrenergic responsiveness. Circ Res 88: 1159–1167.
- View Article
- Google Scholar
140. Yamada KA, Corr PB (1992) Effects of β-adrenergic receptor activation on intracellular calcium and membrane potential in adult cardiac myocytes. J Cardiovasc Electrophysiol 3: 209–224.
- View Article
- Google Scholar
141. MacLennan DH, Kranias EG (2003) Phospholamban: a crucial regulator of cardiac contractility. Nat Rev Mol Cell Biol 4: 566–577.
- View Article
- Google Scholar
142. Eisner D, Bode E, Venetucci L, Trafford A (2013) Calcium flux balance in the heart. J Mol Cell Cardiol 58: 110–117.
- View Article
- Google Scholar
143. Bers DM (2012) Ryanodine receptor S2808 phosphorylation in heart failure. Smoking gun or red herring. Circ Res 110: 796–799.
- View Article
- Google Scholar
144. Marx SO, Reiken S, Hisamatsu Y, Jayaraman T, Burkhoff D, et al. (2000) PKA phosphorylation dissociates FKBP12.6 from the calcium release channel (ryanodine receptor): defective regulation in failing hearts. Cell 101: 365–376.
- View Article
- Google Scholar
145. Zhang H, Makarewich CA, Kubo H, Wang W, Duran JM, et al. (2012) Hyperphosphorylation of the cardiac ryanodine receptor at serine 2808 is not involved in cardiac dysfunction after myocardial infarction. Circ Res 110: 831–840.
- View Article
- Google Scholar
146. Soltis AR, Saucerman JJ (2011) Robustness portraits of diverse biological networks concerved despite order-of-magnitude parameter uncertainty. Bioinformatics 27: 2888–2894.
- View Article
- Google Scholar
147. Rochais F, Abi-Gerges A, Horner K, Lefebvre F, Cooper DMF, et al. (2006) A specific pattern of phosphodiesterases controls the cAMP signals generated by different G_s-coupled receptors in adult rat ventricular myocytes. Circ Res 98: 1081–1088.
- View Article
- Google Scholar
148. Hohl CM, Li Q (1991) Compartmentation of cAMP in adult canine ventricular myocytes: relation to single-cell free Ca²⁺ transients. Circ Res 69: 1369–1379.
- View Article
- Google Scholar

[ref1] 1. Rudy Y, Ackerman MJ, Bers DM, Clancy CE, Houser SR, et al. (2008) System approach to understanding electromechanical activity in the human heart: a National Heart, Lung, and Blood Institute workshop summary. Circulation 118: 1202–1211.
View Article
Google Scholar

[2] View Article

[3] Google Scholar

[ref2] 2. Schaub MC, Hefti MA, Zaugg M (2006) Integration of calcium with the signaling network in cardiac myocytes. J Mol Cell Cardiol 41: 183–214.
View Article
Google Scholar

[5] View Article

[6] Google Scholar

[ref3] 3. Wachter SB, Gilbert EM (2012) Beta-adrenergic receptors, from their discovery and characterization through their manipulation to beneficial clinical application. Cardiology 122: 104–112.
View Article
Google Scholar

[8] View Article

[9] Google Scholar

[ref4] 4. Ho D, Yan L, Iwatsubo K, Vatner DE, Vatner SF (2010) Modulation of β-adrenergic receptor signaling in heart failure and longevity: targeting adenylyl cyclase type 5. Heart Fail Rev 15: 495–512.
View Article
Google Scholar

[11] View Article

[12] Google Scholar

[ref5] 5. Reincober J, Tscheschner H, Pleger ST, Most P, Katus HA, et al. (2012) Targeting GRK2 by gene therapy for heart failure: benefits above β-blockade. Gene Ther 19: 686–693.
View Article
Google Scholar

[14] View Article

[15] Google Scholar

[ref6] 6. Shah AM, Mann DL (2011) In search of new therapeutic targets and strategies for heart failure: recent advances in basic science. Lancet 378: 704–712.
View Article
Google Scholar

[17] View Article

[18] Google Scholar

[ref7] 7. Xiao RP, Zhu W, Zheng M, Chakir K, Bond R, et al. (2004) Subtype-specific β-adrenoceptor signaling pathways in the heart and their potential clinical implications. Trends Pharmacol Sci 25: 358–365.
View Article
Google Scholar

[20] View Article

[21] Google Scholar

[ref8] 8. Heijman J, Volders PGA, Westra RL, Rudy Y (2011) Local control of β-adrenergic stimulation: effects on ventricular myocyte electrophysiology and Ca²⁺ transient. J Mol Cell Cardiol 50: 863–871.
View Article
Google Scholar

[23] View Article

[24] Google Scholar

[ref9] 9. Kuzumoto M, Takeuchi A, Nakai H, Oka C, Noma A, et al. (2008) Simulation analysis of intracellular Na⁺ and Cl⁻ homeostasis during β1-adrenergic stimulation of cardiac myocytes. Prog Biophys Mol Biol 96: 171–186.
View Article
Google Scholar

[26] View Article

[27] Google Scholar

[ref10] 10. Saucerman JJ, Brunton LL, Michailova AP, McCulloch AD (2003) Modeling β-adrenergic control of cardiac myocyte contractility in silico. J Biol Chem 278: 47997–48003.
View Article
Google Scholar

[29] View Article

[30] Google Scholar

[ref11] 11. Saucerman JJ, Healy SN, Belik ME, Puglisi JL, McCulloch AD (2004) Proarrhythmic consequences of a KCNQ1 AKAP-binding domain mutation: computational models of whole cells and heterogeneous tissue. Circ Res 95: 1216–1224.
View Article
Google Scholar

[32] View Article

[33] Google Scholar

[ref12] 12. Yang JH, Saucerman JJ (2012) Phospholemman is a negative feed-forward regulator of Ca²⁺ in β-adrenergic signaling, accelerating β-adrenergic inotropy. J Mol Cell Cardiol 52: 1048–1055.
View Article
Google Scholar

[35] View Article

[36] Google Scholar

[ref13] 13. Iancu RV, Jones SW, Harvey RD (2007) Compartmentation of cAMP signaling in cardiac myocytes: a computational study. Biophys J 92: 3317–3331.
View Article
Google Scholar

[38] View Article

[39] Google Scholar

[ref14] 14. Iancu RV, Ramamurthy G, Warrier S, Nikolaev VO, Lohse MJ, et al. (2008) Cytoplasmic cAMP concentrations in intact cardiac myocytes. Am J Physiol Cell Physiol 295: C414–C422.
View Article
Google Scholar

[41] View Article

[42] Google Scholar

[ref15] 15. Maguy A, Hebert TE, Nattel S (2006) Involvement of lipid rafts and caveolae in cardiac ion channel function. Cardiovasc Res 69: 798–807.
View Article
Google Scholar

[44] View Article

[45] Google Scholar

[ref16] 16. Balijepalli RC, Kamp TJ (2008) Caveolae, ion channels and cardiac arrhythmias. Prog Biophys Mol Biol 98: 149–160.
View Article
Google Scholar

[47] View Article

[48] Google Scholar

[ref17] 17. Harvey RD, Calaghan SC (2012) Caveolae create local signalling domains through their distinct protein content, lipid profile and morphology. J Mol Cell Cardiol 52: 366–375.
View Article
Google Scholar

[50] View Article

[51] Google Scholar

[ref18] 18. Weiss S, Oz S, Benmocha A, Dascal N (2013) Regulation of cardiac L-type Ca²⁺ channel Ca_V1.2 via the β-adrenergic-cAMP-protein kinase A pathway. Old dogmas, advances, and new uncertainties. Circ Res 113: 617–631.
View Article
Google Scholar

[53] View Article

[54] Google Scholar

[ref19] 19. Balijepalli RC, Foell JD, Hall DD, Hell JW, Kamp TJ (2006) Localization of cardiac L-type Ca²⁺ channels to a caveolar macromolecular signaling complex is required for β₂-adrenergic regulation. Proc Natl Acad Sci USA 103: 7500–7505.
View Article
Google Scholar

[56] View Article

[57] Google Scholar

[ref20] 20. Rybin VO, Xu X, Lisanti MP, Steinberg SF (2000) Differential targeting of β-adrenergic receptor subtypes and adenylyl cyclase to cardiomyocyte caveolae: a mechanism to functionally regulate the cAMP signaling pathway. J Biol Chem 275: 41447–41457.
View Article
Google Scholar

[59] View Article

[60] Google Scholar

[ref21] 21. Scriven DRL, Asghari P, Schulson MN, Moore EDW (2010) Analysis of Ca_V1.2 and ryanodine receptor clusters in rat ventricular myocytes. Biophys J 99: 3923–3929.
View Article
Google Scholar

[62] View Article

[63] Google Scholar

[ref22] 22. Best JM, Kamp TJ (2012) Different subcellular populations of L-type Ca²⁺ channels exhibit unique regulation and functional roles in cardiomyocytes. J Mol Cell Cardiol 52: 376–387.
View Article
Google Scholar

[65] View Article

[66] Google Scholar

[ref23] 23. Engelhardt S, Hein L, Wiesmann F, Lohse MJ (1999) Progressive hypertrophy and heart failure in β₁-adrenergic receptor transgenic mice. Proc Natl Acad Sci USA 96: 7059–7064.
View Article
Google Scholar

[68] View Article

[69] Google Scholar

[ref24] 24. Milano CA, Allen LF, Rockman HA, Dolber PC, McMinn TR, et al. (1994) Enhanced myocardial function in transgenic mice overexpressing the β₂-adrenergic receptor. Science 264: 582–586.
View Article
Google Scholar

[71] View Article

[72] Google Scholar

[ref25] 25. Bondarenko VE, Szigeti GP, Bett GCL, Kim SJ, Rasmusson RL (2004) Computer model of action potential; of mouse ventricular myocytes. Am J Physiol Heart Circ Physiol 287: H1378–H1403.
View Article
Google Scholar

[74] View Article

[75] Google Scholar

[ref26] 26. Petkova-Kirova PS, London B, Salama G, Rasmusson RL, Bondarenko VE (2012) Mathematical modeling mechanisms of arrhythmias in transgenic mouse heart overexpressing TNF-α. Am J Physiol Heart Circ Physiol 302: H934–H952.
View Article
Google Scholar

[77] View Article

[78] Google Scholar

[ref27] 27. Bers DM (2001) Excitation-Contraction Coupling and Cardiac Contractile Force (2^nd ed.). Dordrecht, The Netherlands: Kluwer Academic. 427 p.

[ref28] 28. Steinberg SF (2004) β₂-adrenergic receptor signaling complexes in cardiomyocyte caveolae/lipid rafts. J Mol Cell Cardiol 37: 407–415.
View Article
Google Scholar

[81] View Article

[82] Google Scholar

[ref29] 29. Hilal-Dandan R, Kanter JR, Brunton LL (2000) Characterization of G-protein signaling in ventricular myocytes from the adult mouse heart: differences from the rat. J Mol Cell Cardiol 32: 1211–1221.
View Article
Google Scholar

[84] View Article

[85] Google Scholar

[ref30] 30. Nikolaev VO, Moshkov A, Lyon AR, Miragoli M, Noval P, et al. (2010) β₂-adrenergic receptor redistribution in heart failure changes cAMP compartmentation. Science 327: 1653–1657.
View Article
Google Scholar

[87] View Article

[88] Google Scholar

[ref31] 31. Lohse MJ, Hein P, Hoffmann C, Nikolaev VO, Vilardaga JP, et al. (2008) Kinetics of G-protein-coupled receptor signals in intact cells. Br J Pharmacol 153: S125–S132.
View Article
Google Scholar

[90] View Article

[91] Google Scholar

[ref32] 32. Freedman NJ, Liggett SB, Drachman DE, Pei G, Caron MG, et al. (1995) Phosphorylation and desensitization of the human β₁-adrenergic receptor: involvement of G protein-coupled receptor kinases and cAMP-dependent protein kinase. J Biol Chem 270: 17953–17961.
View Article
Google Scholar

[93] View Article

[94] Google Scholar

[ref33] 33. Göttle M, Geduhn J, König B, Gille A, Höcherl K, et al. (2009) Characterization of mouse heart adenylyl cyclase. J Pharmacol Exp Ther 329: 1156–1165.
View Article
Google Scholar

[96] View Article

[97] Google Scholar

[ref34] 34. Tang T, Gao MH, Lai NC, Firth AL, Takahashi T, et al. (2008) Adenylyl cyclase type 6 deletion decreases left ventricular function via impaired calcium handling. Circulation 117: 61–69.
View Article
Google Scholar

[99] View Article

[100] Google Scholar

[ref35] 35. Head BP, Patel HH, Roth DM, Lai NC, Niesman IR, et al. (2005) G-protein-coupled receptor signaling components localize in both sarcolemmal and intracellular caveolin-3-associated microdomains in adult cardiac myocytes. J Biol Chem 280: 31036–31044.
View Article
Google Scholar

[102] View Article

[103] Google Scholar

[ref36] 36. Ostrom RS, Insel PA (2004) The evolving role of lipid rafts and caveolae in G protein-coupled receptor signaling: implications for molecular pharmacology. Br J Pharmacol 143: 235–245.
View Article
Google Scholar

[105] View Article

[106] Google Scholar

[ref37] 37. Chen-Goodspeed M, Lukan AN, Dessauer CW (2005) Modeling of Gα_s and Gα_i regulation of human type V and VI adenylyl cyclase. J Biol Chem 280: 1808–1816.
View Article
Google Scholar

[108] View Article

[109] Google Scholar

[ref38] 38. Gao B, Gilman AG (1991) Cloning and expression of a widely distributed (type IV) adenylyl cyclase. Proc Natl Acad Sci USA 88: 10178–10182.
View Article
Google Scholar

[111] View Article

[112] Google Scholar

[ref39] 39. Gao X, Sadana R, Dessauer CW, Patel TB (2007) Conditional stimulation of type V and VI adenylyl cyclases by G protein βγ subunits. J Biol Chem 282: 294–302.
View Article
Google Scholar

[114] View Article

[115] Google Scholar

[ref40] 40. Zimmermann G, Taussig R (1996) Protein kinase C alters the responsiveness of adenylyl cyclases to G protein α and βγ subunits. J Biol Chem 271: 27161–27166.
View Article
Google Scholar

[117] View Article

[118] Google Scholar

[ref41] 41. Post SR, Hilal-Dandan R, Urasawa K, Brunton LL, Insel PA (1995) Quantification of signaling components and amplification in the β-adrenergic-receptor-adenylyl cyclase pathway in isolated adult rat ventricular myocytes. Biochem J 311: 75–80.
View Article
Google Scholar

[120] View Article

[121] Google Scholar

[ref42] 42. Tepe NM, Liggett SB (1999) Transgenic replacement of type V adenylyl cyclase identifies a critical mechanism of β-adrenergic receptor dysfunction in the G_αq overexpressing mouse. FEBS Lett 458: 236–240.
View Article
Google Scholar

[123] View Article

[124] Google Scholar

[ref43] 43. Lemire I, Allen BG, Rindt H, Hebert TE (1998) Cardiac-specific overexpression of α_1BAR regulates βAR activity via molecular crosstalk. J Mol Cell Cardiol 30: 1827–1839.
View Article
Google Scholar

[126] View Article

[127] Google Scholar

[ref44] 44. Richter W, Xie M, Scheitrum C, Krall J, Movsesian MA, et al. (2011) Conserved expression and functions of PDE4 in rodent and human heart. Basic Res Cardiol 106: 249–262.
View Article
Google Scholar

[129] View Article

[130] Google Scholar

[ref45] 45. Bode DC, Kanter JR, Brunton LL (1991) Cellular distribution of phosphodiesterase isoforms in rat cardiac tissue. Circ Res 68: 1070–1079.
View Article
Google Scholar

[132] View Article

[133] Google Scholar

[ref46] 46. Fischmeister R, Castro LRV, Abi-Gerges A, Rochais F, Jurevičius J, et al. (2006) Compartmentation of cyclic nucleotide signaling in the heart: the role of cyclic nucleotide phosphodiesterases. Circ Res 99: 816–828.
View Article
Google Scholar

[135] View Article

[136] Google Scholar

[ref47] 47. Osadchii OE (2007) Myocardial phosphodiesterases and regulation of cardiac contractility in health and cardiac disease. Cardiovasc Drugs Ther 21: 171–194.
View Article
Google Scholar

[138] View Article

[139] Google Scholar

[ref48] 48. Mongillo M, Tocchetti CG, Terrin A, Lissandron V, Cheung YF, et al. (2006) Compartmentalized phosphodiesterase-2 activity blunts β-adrenergic cardiac inotropy via an NO/cGMP-dependent pathway. Circ Res 98: 226–234.
View Article
Google Scholar

[141] View Article

[142] Google Scholar

[ref49] 49. Georget M, Mateo P, Vandecasteele G, Lipskaia L, Defer N, et al. (2003) Cyclic AMP compartmentation due to increase cAMP-phosphodiesterase activity in transgenic mice with a cardiac-directed expression of the human adenylyl cyclase type 8 (AC8). FASEB J 17: 1380–1391.
View Article
Google Scholar

[144] View Article

[145] Google Scholar

[ref50] 50. Adams SR, Harootunian AT, Buechler YJ, Taylor SS, Tsien RY (1991) Fluorescence ratio imaging of cyclic AMP in single cell. Nature 349: 694–697.
View Article
Google Scholar

[147] View Article

[148] Google Scholar

[ref51] 51. Dostmann WRG, Taylor SS (1991) Identifying the molecular switches that determine whether (R_p)-cAMPS functions as an antagonist or an agonist in the activation of cAMP-dependent protein kinase I. Biochemistry. 30: 8710–8716.
View Article
Google Scholar

[150] View Article

[151] Google Scholar

[ref52] 52. Lin F, Owens A, Chen S, Stevens ME, Kesteven S, et al. (2001) Targeted α_1A-adrenergic receptor overexpression induces enhanced cardiac contractility but not hypertrophy. Circ Res 89: 343–350.
View Article
Google Scholar

[153] View Article

[154] Google Scholar

[ref53] 53. Roman BB, Goldspink PH, Spaite E, Urboniene D, McKinney R, et al. (2004) Inhibition of PKC phosphorylation of TnI improves cardiac performance in vivo. Am J Physiol Heart Circ Physiol 286: H2089–H2095.
View Article
Google Scholar

[156] View Article

[157] Google Scholar

[ref54] 54. Beavo JA, Bechtel PJ, Krebs EG (1974) Activation of protein kinase by physiological concentrations of cyclic AMP. Proc Natl Acad Sci USA 71: 3580–3583.
View Article
Google Scholar

[159] View Article

[160] Google Scholar

[ref55] 55. Dao KK, Teigen K, Kopperud R, Hodneland E, Schwede F, et al. (2006) Epac1 and cAMP-dependent protein kinase holoenzyme have similar cAMP affinity, but their cAMP domains have distinct structural features and cyclic nucleotide recognition. J Biol Chem 281: 21500–21511.
View Article
Google Scholar

[162] View Article

[163] Google Scholar

[ref56] 56. Hofmann F, Beavo JA, Bechtel PJ, Krebs EG (1975) Comparison of adenosine 3′: 5′-monophosphate-dependent protein kinase from rabbit skeletal and bovine heart muscle. J Biol Chem 250: 7795–7801.
View Article
Google Scholar

[165] View Article

[166] Google Scholar

[ref57] 57. Buxton ILO, Brunton LL (1983) Compartments of cyclic AMP and protein kinase in mammalian cardiomyocytes. J Biol Chem 258: 10233–10239.
View Article
Google Scholar

[168] View Article

[169] Google Scholar

[ref58] 58. Hescheler J, Kameyama M, Trautwein W, Mieskes G, Söling HD (1987) Regulation of the cardiac calcium channel by protein phosphatases. Eur J Biochem 165: 261–266.
View Article
Google Scholar

[171] View Article

[172] Google Scholar

[ref59] 59. MacDougall LK, Jones LR, Cohen P (1991) Identification of the major protein phosphatases in mammalian cardiac muscle which dephosphorylate phospholamban. Eur J Biochem 196: 725–734.
View Article
Google Scholar

[174] View Article

[175] Google Scholar

[ref60] 60. Neumann J, Boknik P, Herzig S, Schmitz W, Scholz H, et al. (1993) Evidence for physiological functions of protein phosphatases in the heart: evaluation with okadaic acid. Am J Physiol Heart Circ Physiol 265: H257–H266.
View Article
Google Scholar

[177] View Article

[178] Google Scholar

[ref61] 61. duBell WH, Gigena MS, Guatimosim S, Long X, Lederer WJ, et al. (2002) Effects of PP1/PP2A inhibitor calyculin A on the E-C coupling cascade in murine ventricular myocytes. Am J Physiol Heart Circ Physiol 282: H38–H48.
View Article
Google Scholar

[180] View Article

[181] Google Scholar

[ref62] 62. Müller FU, Lewin G, Baba HA, Boknik P, Fabritz L, et al. (2005) Heart-directed expression of a human cardiac isoform of cAMP-response element modulator in transgenic mice. J Biol Chem 280: 6906–6914.
View Article
Google Scholar

[183] View Article

[184] Google Scholar

[ref63] 63. Herzig S, Neumann J (2000) Effects of serine/threonine protein phosphatases on ion channels in excitable membranes. Physiol Rev 80: 173–210.
View Article
Google Scholar

[186] View Article

[187] Google Scholar

[ref64] 64. Carr AN, Schmidt AG, Suzuki Y, del Monte F, Sato Y, et al. (2002) Type 1 phosphatase, a negative regulator of cardiac function. Mol Cell Biol 22: 4124–4135.
View Article
Google Scholar

[189] View Article

[190] Google Scholar

[ref65] 65. El-Armouche A, Wittköpper K, Degenhardt F, Weinberger F, Didié M, et al. (2008) Phosphatase inhibitor-1-deficient mice are protected from catecholamine-induced arrhythmias and myocardial hypertrophy. Cardiovasc Res 80: 396–406.
View Article
Google Scholar

[192] View Article

[193] Google Scholar

[ref66] 66. Nicolaou P, Hajjar RJ, Kranias EG (2009) Role of protein phosphatase-1 inhibitor-1 in cardiac physiology and pathophysiology. J Mol Cell Cardiol 47: 365–371.
View Article
Google Scholar

[195] View Article

[196] Google Scholar

[ref67] 67. Neumann J, Gupta RC, Schmitz W, Scholz H, Nairn AC, et al. (1991) Evidence for isoproterenol-induced phosphorylation of phosphatase inhibitor-1 in the intact heart. Circ Res 69: 1450–1457.
View Article
Google Scholar

[198] View Article

[199] Google Scholar

[ref68] 68. O’Connell TD, Ni YG, Lin KM, Han H, Yan Z (2003) Isolation and culture of adult mouse cardiac myocytes for signaling studies. AfCS Research Reports 1: CM0005.
View Article
Google Scholar

[201] View Article

[202] Google Scholar

[ref69] 69. Shibata EF, Brown TLY, Washburn ZW, Bai J, Revak TJ, et al. (2006) Autonomic regulation of voltage-gated cardiac ion channels. J Cardiovasc Electrophysiol (Suppl 1): S34–S42.

[ref70] 70. Makarewich CA, Correll RN, Gao H, Zhang H, Yang B, et al. (2012) A caveolae-targeted L-type Ca²⁺ channel antagonist inhibits hypertrophic signaling without reducing cardiac contractility. Circ Res 110: 669–674.
View Article
Google Scholar

[205] View Article

[206] Google Scholar

[ref71] 71. Chu G, Luo W, Slack JP, Tilgmann C, Sweet WE, et al. (1996) Compensatory mechanisms associated with the hyperdynamic function of phospholamban-deficient mouse hearts. Circ Res 79: 1064–1076.
View Article
Google Scholar

[208] View Article

[209] Google Scholar

[ref72] 72. Bers DM, Stiffel VM (1993) Ratio of ryanodine to dihydropyridine receptors in cardiac and skeletal muscle and implications for E-C coupling. Am J Physiol Cell Physiol 264: C1587–C1593.
View Article
Google Scholar

[211] View Article

[212] Google Scholar

[ref73] 73. Bracken N, ElKadri M, Hart G, Hussain M (2006) The role of constitutive PKA-mediated phosphorylation in the regulation of basal I_Ca in isolated rat cardiac myocytes. Br J Pharmacol 148: 1108–1115.
View Article
Google Scholar

[214] View Article

[215] Google Scholar

[ref74] 74. Tang M, Zhang X, Li Y, Guan Y, Ai X, et al. (2010) Enhanced basal contractility but reduced excitation-contraction coupling efficiency and β-adrenergic reserve of hearts with increased Cav1.2 activity. Am J Physiol Heart Circ Physiol 299: H519–H528.
View Article
Google Scholar

[217] View Article

[218] Google Scholar

[ref75] 75. Wang H, Kohr MJ, Wheeler DG, Ziolo MT (2008) Endothelial nitric oxide synthase decreases β-adrenergic responsiveness via inhibition of the L-type Ca²⁺ current. Am J Physiol Heart Circ Physiol 294: H1473–H1480.
View Article
Google Scholar

[220] View Article

[221] Google Scholar

[ref76] 76. Tsien RW, Bean BP, Hess P, Lansman JB, Nilius B, et al. (1986) Mechanisms of calcium channel modulation by β-adrenergic agents and dihydropyridine calcium agonists. J Mol Cell Cardiol 18: 691–710.
View Article
Google Scholar

[223] View Article

[224] Google Scholar

[ref77] 77. Hulme JT, Westenbroek RE, Scheuer T, Catterall WA (2006) Phosphorylation of serine 1928 in the distal C-terminal domain of cardiac Ca_v1.2 channels during β1-adrenergic regulation. Proc Natl Acad Sci USA 103: 16574–16579.
View Article
Google Scholar

[226] View Article

[227] Google Scholar

[ref78] 78. Kameyama M, Hescheler J, Hofmann F, Trautwein W (1986) Modulation of Ca current during the phosphorylation cycle in the guinea pig heart. Pflügers Arch 407: 123–128.
View Article
Google Scholar

[229] View Article

[230] Google Scholar

[ref79] 79. Kim SJ, Yatani A, Vatner DE, Yamamoto S, Ishikawa Y, et al. (1999) Differential regulation of inotropy and lusitropy in overexpressed Gsα myocytes through cAMP and Ca²⁺ channel pathways. J Clin Invest 103: 1089–1097.
View Article
Google Scholar

[232] View Article

[233] Google Scholar

[ref80] 80. Sako H, Green SA, Kranias EG, Yatani A (1997) Modulation of cardiac Ca²⁺ channels by isoproterenol studied in transgenic mice with altered SR Ca²⁺ content. Am J Physiol Cell Physiol 273: C1666–C1672.
View Article
Google Scholar

[235] View Article

[236] Google Scholar

[ref81] 81. Mitarai S, Reed TD, Yatani A (2000) Changes in ionic currents and β-adrenergic receptor signaling in hypertrophied myocytes overexpressing Gα_q. Am J Physiol Heart Circ Physiol 279: H139–H148.
View Article
Google Scholar

[238] View Article

[239] Google Scholar

[ref82] 82. Yarbrough TL, Lu T, Lee HC, Shibata EF (2002) Localization of cardiac sodium channels in caveolin-rich membrane domains. Regulation of sodium current amplitude. Circ Res 90: 443–449.
View Article
Google Scholar

[241] View Article

[242] Google Scholar

[ref83] 83. Palygin OA, Pettus JM, Shibata EF (2008) Regulation of caveolar cardiac sodium current by a single G_sα histidine residue. Am J Physiol Heart Circ Physiol 294: H1693–H1699.
View Article
Google Scholar

[244] View Article

[245] Google Scholar

[ref84] 84. Kirstein M, Eickhorn R, Kochsiek K, Langenfeld H (1996) Dose-dependent alteration of rat cardiac sodium current by isoproterenol: results from direct measurements on multicellular preparations. Pflügers Arch 431: 395–401.
View Article
Google Scholar

[247] View Article

[248] Google Scholar

[ref85] 85. Matsuda JJ, Lee HC, Shibata EF (1993) Acetylcholine reversal of isoproterenol-stimulated sodium currents in rabbit ventricular myocytes. Circ Res 72: 517–525.
View Article
Google Scholar

[250] View Article

[251] Google Scholar

[ref86] 86. Baba S, Dun W, Boyden PA (2004) Can PKA activators rescue Na⁺ channel function in epicardial border zone cells that survive in the infarcted canine heart? Cardiovasc Res 64: 260–267.
View Article
Google Scholar

[253] View Article

[254] Google Scholar

[ref87] 87. Ono K, Fozzard HA, Hanck DA (1993) Mechanism of cAMP-dependent modulation of cardiac sodium channel current kinetics. Circ Res 72: 807–815.
View Article
Google Scholar

[256] View Article

[257] Google Scholar

[ref88] 88. Zhou J, Yi J, Hu NN, George AL Jr, Murray KT (2000) Activation of protein kinase A modulates trafficking of the human cardiac sodium channel in Xenopus oocytes. Circ Res 87: 33–38.
View Article
Google Scholar

[259] View Article

[260] Google Scholar

[ref89] 89. Rook MB, Evers MM, Vos MA, Bierhuizen MFA (2012) Biology of cardiac sodium channel Na_v1.5 expression. Cardiovasc Res 93: 12–23.
View Article
Google Scholar

[262] View Article

[263] Google Scholar

[ref90] 90. Clancy CE, Rudy Y (2002) Na⁺ channel mutation that causes both Brugada and long-QT syndrome phenotypes: a simulation study of mechanism. Circulation 105: 1208–1213.
View Article
Google Scholar

[265] View Article

[266] Google Scholar

[ref91] 91. Jayasinghe ID, Cannell MB, Soeller C (2009) Organization of ryanodine receptors, transverse tubules, and sodium-calcium exchanger in rat myocytes. Biophys J 97: 2664–2673.
View Article
Google Scholar

[268] View Article

[269] Google Scholar

[ref92] 92. Wong J, Baddeley D, Bushong EA, Yu Z, Ellisman MH, et al. (2013) Nanoscale distribution of ryanodine receptors and caveolin-3 in mouse ventricular myocytes: Dilation of t-tubules near junctions. Biophys J 104: L22–L24.
View Article
Google Scholar

[271] View Article

[272] Google Scholar

[ref93] 93. Xiao B, Tian X, Xie W, Jones PP, Cai S, et al. (2007) Functional consequence of protein kinase A-dependent phosphorylation of the cardiac ryanodine receptor: sensitization of store overload-induced Ca²⁺ release. J Biol Chem 282: 30256–30264.
View Article
Google Scholar

[274] View Article

[275] Google Scholar

[ref94] 94. Xiao B, Zhong G, Obayashi M, Yang D, Chen K, et al. (2006) Ser-2030, but not Ser-2808, is the major phosphorylation site in cardiac ryanodine receptors responding to protein kinase A activation upon β-adrenergic stimulation in normal and failing hearts. Biochem J 396: 7–16.
View Article
Google Scholar

[277] View Article

[278] Google Scholar

[ref95] 95. Takasago T, Imagawa T, Furukawa KI, Ogurusu T, Shigekawa M (1991) Regulation of the cardiac ryanodine receptor by protein kinase-dependent phosphorylation. J Biochem 109: 163–170.
View Article
Google Scholar

[280] View Article

[281] Google Scholar

[ref96] 96. Xiao J, Tian X, Jones PP, Bolstad J, Kong H, et al. (2007) Removal of FKBP12.6 does not alter the conductance and activation of the cardiac ryanodine receptor or the susceptibility to stress-induced ventricular arrhythmias. J Biol Chem 282: 34828–34838.
View Article
Google Scholar

[283] View Article

[284] Google Scholar

[ref97] 97. Liu L, Askari A (2006) β-Subunit of cardiac Na⁺-K⁺-ATPase dictates the concentration of the functional enzyme in caveolae. Am J Physiol Cell Physiol 291: C569–C578.
View Article
Google Scholar

[286] View Article

[287] Google Scholar

[ref98] 98. Fuller W, Eaton P, Medina RA, Bell J, Shattock MJ (2001) Differential centrifugation separates cardiac sarcolemmal and endosomal membranes from Langendorff-perfused rat hearts. Anal Biochem 293: 216–223.
View Article
Google Scholar

[289] View Article

[290] Google Scholar

[ref99] 99. Fuller W, Tulloch LB, Shattock MJ, Calaghan SC, Howie J, et al. (2013) Regulation of the cardiac sodium pump. Cell Mol Life Sci 70: 1357–1380.
View Article
Google Scholar

[292] View Article

[293] Google Scholar

[ref100] 100. Despa S, Bossuyt J, Han F, Ginsburg KS, Jia LG, et al. (2005) Phospholemman-phosphorylation mediates the β-adrenergic effects on Na/K pump function in cardiac myocytes. Circ Res 97: 252–259.
View Article
Google Scholar

[295] View Article

[296] Google Scholar

[ref101] 101. Gao J, Mathias RT, Cohen IS, Baldo GJ (1992) Isoprenaline, Ca²⁺ and the Na⁺-K⁺ pump in guinea-pig ventricular myocytes. J Physiol 449: 689–704.
View Article
Google Scholar

[298] View Article

[299] Google Scholar

[ref102] 102. Abi-Char J, Maguy A, Coulombe A, Balse E, Ratajczak P, et al. (2007) Membrane cholesterol modulates Kv1.5 potassium channel distribution and function in rat cardiomyocytes. J Physiol 582: 1205–1217.
View Article
Google Scholar

[301] View Article

[302] Google Scholar

[ref103] 103. Ravens U, Wettwer E (2011) Ultra-rapid delayed rectifier channels: molecular basis and therapeutic implications. Cardiovasc Res 89: 776–785.
View Article
Google Scholar

[304] View Article

[305] Google Scholar

[ref104] 104. Folco EJ, Liu GX, Koren G (2004) Caveolin-3 and SAP97 form a scaffolding protein complex that regulates the voltage-gated potassium channel Kv1.5. Am J Physiol Heart Circ Physiol 287: H681–H690.
View Article
Google Scholar

[307] View Article

[308] Google Scholar

[ref105] 105. Martens JR, Sakamoto N, Sullivan SA, Grobaski TD, Tamkun MM (2001) Isoform-specific localization of voltage-gated K⁺ channels to distinct lipid raft populations: targeting of Kv1.5 to caveolae. J Biol Chem 276: 8409–8414.
View Article
Google Scholar

[310] View Article

[311] Google Scholar

[ref106] 106. Martínez-Mármol R, Villalonga N, Solé L, Vicente R, Tamkun MM, et al. (2008) Multiple Kv1.5 targeting to membrane surface microdomains. J Cell Physiol 217: 667–673.
View Article
Google Scholar

[313] View Article

[314] Google Scholar

[ref107] 107. Li GR, Feng J, Wang Z, Fermini B, Nattel S (1996) Adrenergic modulation of ultrarapid delayed rectifier K⁺ current in human atrial myocytes. Circ Res 78: 903–915.
View Article
Google Scholar

[316] View Article

[317] Google Scholar

[ref108] 108. Yue L, Feng J, Wang Z, Nattel S (1999) Adrenergic control of the ultrarapid delayed rectifier current in canine atrial myocytes. J Physiol 516: 385–398.
View Article
Google Scholar

[319] View Article

[320] Google Scholar

[ref109] 109. González de la Fuente M, Barana A, Gόmez R, Amorόs I, Dolz-Gaitόn P, et al. (2013) Chronic atrial fibrillation up-regulates β1-adrenoceptors affecting repolarizing currents and action potential duration. Cardiovasc Res 97: 379–388.
View Article
Google Scholar

[322] View Article

[323] Google Scholar

[ref110] 110. Hoffman DA, Johnson D (1998) Downregulation of transient K⁺ channels in dendrites of hippocampal CA1 pyramidal neurons by activation of PKA and PKC. J Neurosci 18: 3521–3528.
View Article
Google Scholar

[325] View Article

[326] Google Scholar

[ref111] 111. Zhang M, Fei XW, He YL, Yang G, Mei YA (2009) Bradykinin inhibits the transient outward K⁺ current in mouse Schwann cells via the cAMP/PKA pathway. Am J Physiol Cell Physiol 296: C1364–C1372.
View Article
Google Scholar

[328] View Article

[329] Google Scholar

[ref112] 112. Anumonwo JMB, Lopatin AN (2010) Cardiac strong inward rectifier potassium channels. J Mol Cell Cardiol 48: 45–54.
View Article
Google Scholar

[331] View Article

[332] Google Scholar

[ref113] 113. Vaidyanathan R, Taffet SM, Vikstrom KL, Anumonwo JMB (2010) Regulation of cardiac inward rectifier potassium current (I_K1) by synapse-associated protein-97. J Biol Chem 285: 28000–28009.
View Article
Google Scholar

[334] View Article

[335] Google Scholar

[ref114] 114. Simmerman HKB, Jones LR (1998) Phospholamban: protein structure, mechanism of action, and role in cardiac function. Physiol Rev 78: 921–947.
View Article
Google Scholar

[337] View Article

[338] Google Scholar

[ref115] 115. Wolska BM (2009) Calcineurin and cardiac function: is more or less better for the heart? Am J Physiol Heart Circ Physiol 297: H1576–H1577.
View Article
Google Scholar

[340] View Article

[341] Google Scholar

[ref116] 116. Karczewski P, Bartel S, Krause EG (1990) Differential sensitivity to isoprenaline of troponin I and phospholamban phosphorylation in isolated rat hearts. Biochem J 266: 115–122.
View Article
Google Scholar

[343] View Article

[344] Google Scholar

[ref117] 117. Kuschel M, Karczewski P, Hempel P, Schlegel WP, Krause EG, et al. (1999) Ser¹⁶ prevails over Thr¹⁷ phospholamban phosphorylation in the β-adrenergic regulation of cardiac relaxation. Am J Physiol Heart Circ Physiol 276: H1625–H1633.
View Article
Google Scholar

[346] View Article

[347] Google Scholar

[ref118] 118. Li L, Desantiago J, Chu G, Kranias EG, Bers DM (2000) Phosphorylation of phospholamban and troponin I in β-adrenergic-induced acceleration of cardiac relaxation. Am J Physiol Heart Circ Physiol 278: H769–H779.
View Article
Google Scholar

[349] View Article

[350] Google Scholar

[ref119] 119. Lindemann JP, Jones LR, Hathaway DR, Henry BG, Watanabe AM (1983) β-adrenergic stimulation of phospholamban phosphorylation and Ca²⁺-ATPase activity in guinea pig ventricles. J Biol Chem 258: 464–471.
View Article
Google Scholar

[352] View Article

[353] Google Scholar

[ref120] 120. Sulakhe PV, Vo XT (1995) Regulation of phospholamban and troponin-I phosphorylation in the intact rat cardiomyocytes by adrenergic and cholinergic stimuli: roles of cyclic nucleotides, calcium, protein kinases and phosphatases and depolarization. Mol Cell Biochem 149/150: 103–126.
View Article
Google Scholar

[355] View Article

[356] Google Scholar

[ref121] 121. Robertson SP, Johnson JD, Holroyde MJ, Kranias EG, Potter JD, et al. (1982) The effect of troponin I phosphorylation on the Ca²⁺-binding properties of the Ca²⁺-regulatory site of bovine cardiac troponin. J Biol Chem 257: 260–263.
View Article
Google Scholar

[358] View Article

[359] Google Scholar

[ref122] 122. Bondarenko VE, Bett GCL, Rasmusson RL (2004) A model of graded calcium release and L-type Ca²⁺ channel inactivation in cardiac muscle. Am J Physiol Heart Circ Physiol 286: H1154–H1169.
View Article
Google Scholar

[361] View Article

[362] Google Scholar

[ref123] 123. Leroy J, Abi-Gerges A, Nikolaev VO, Richter W, Lechêne P, et al. (2008) Spatiotemporal dynamics of β-adrenergic cAMP signals and L-type Ca²⁺ channel regulation in adult rat ventricular myocytes: role of phosphodiesterases. Circ Res 102: 1091–1100.
View Article
Google Scholar

[364] View Article

[365] Google Scholar

[ref124] 124. Mongillo M, McSorley T, Evellin S, Sood A, Lissandron V, et al. (2004) Fluorescence resonance energy transfer-based analysis of cAMP dynamics in live neonatal rat cardiac myocytes reveals distinct functions of compartmentalized phosphodiesterases. Circ Res 95: 67–75.
View Article
Google Scholar

[367] View Article

[368] Google Scholar

[ref125] 125. Tong XY, Porter LM, Liu GX, Dhar-Chowdhury P, Srivastava S, et al. (2006) Consequences of cardiac myocyte-specific ablation of K_ATP channels in transgenic mice expressing dominant negative Kir6 subunits. Am J Physiol Heart Circ Physiol 291: H543–H551.
View Article
Google Scholar

[370] View Article

[371] Google Scholar

[ref126] 126. Wu Y, Temple J, Zhang R, Dzhura I, Zhang W, et al. (2002) Calmodulin kinase II and arrhythmias in a mouse model of cardiac hypertrophy. Circulation 106: 1288–1293.
View Article
Google Scholar

[373] View Article

[374] Google Scholar

[ref127] 127. Despa S, Tucker AL, Bers DM (2008) Phospholemman-mediated activation of Na/K-ATPase limits [Na]_i and inotropic state during β-adrenergic stimulation in mouse ventricular myocytes. Circulation 117: 1849–1855.
View Article
Google Scholar

[376] View Article

[377] Google Scholar

[ref128] 128. Knollmann BC, Kirchhof P, Sirenko SG, Degen H, Greene AE, et al. (2003) Familial hypertrophic cardiomyopathy-linked mutant troponin T causes stress-induced ventricular tachycardia and Ca²⁺-dependent action potential remodeling. Circ Res 92: 428–436.
View Article
Google Scholar

[379] View Article

[380] Google Scholar

[ref129] 129. Liu N, Denegri M, Ruan Y, Avelino-Cruz JE, Perissi A, et al. (2011) Short communication: Flecainide exerts an antiarrhythmic effect in a mouse model of catecholaminergic polymorphic ventricular tachycardia by increasing the threshold for triggered activity. Circ Res 109: 291–295.
View Article
Google Scholar

[382] View Article

[383] Google Scholar

[ref130] 130. Song J, Gao E, Wang JF, Zhang XQ, Chan TO, et al. (2012) Constitutive overexpression of phosphomimetic phospholemman S68E mutant results in arrhythmias, early mortality, and heart failure: potential involvement of Na⁺/Ca²⁺ exchanger. Am J Physiol Heart Circ Physiol 302: H770–H781.
View Article
Google Scholar

[385] View Article

[386] Google Scholar

[ref131] 131. Benkusky NA, Weber CS, Scherman JA, Farrell EF, Hacker TA, et al. (2007) Intact β-adrenergic response and unmodified progression toward heart failure in mice with genetic ablation of a major protein kinase A phosphorylation site in the cardiac ryanodine receptor. Circ Res 101: 819–829.
View Article
Google Scholar

[388] View Article

[389] Google Scholar

[ref132] 132. Fernández-Velasco M, Rueda A, Rizzi N, Benitah JP, Colombi B, et al. (2009) Increased Ca²⁺ sensitivity of the ryanodine receptor mutant RyR2^R4496C underlies catecholaminergic polymorphic ventricular tachycardia. Circ Res 104: 201–209.
View Article
Google Scholar

[391] View Article

[392] Google Scholar

[ref133] 133. Despa S, Bers DM (2013) Na⁺ transport in the normal and failing heart – Remember the balance. J Mol Cell Cardiol 61: 2–10.
View Article
Google Scholar

[394] View Article

[395] Google Scholar

[ref134] 134. Xiao RP, Avdonin P, Zhou YY, Cheng H, Akhter SA, et al. (1999) Coupling of β₂-adrenoceptor to G_i proteins and its physiological relevance in murine cardiac myocytes. Circ Res 84: 43–52.
View Article
Google Scholar

[397] View Article

[398] Google Scholar

[ref135] 135. Bers DM (2002) Cardiac excitation-contraction coupling. Nature 415: 198–205.
View Article
Google Scholar

[400] View Article

[401] Google Scholar

[ref136] 136. Bondarenko VE, Rasmusson RL (2010) Transmural heterogeneity of repolarization and Ca²⁺ handling in a model of mouse ventricular tissue. Am J Physiol Heart Circ Physiol 299: H454–H469.
View Article
Google Scholar

[403] View Article

[404] Google Scholar

[ref137] 137. Bondarenko VE, Rasmusson RL (2007) Simulations of propagated mouse ventricular action potentials: effects of molecular heterogeneity. Am J Physiol Heart Circ Physiol 293: H1816–H1832.
View Article
Google Scholar

[406] View Article

[407] Google Scholar

[ref138] 138. Volders PGA, Stengl M, van Opstal JM, Gerlach U, Spätjens RLHMG, et al. (2003) Probing the contribution of I_Ks to canine ventricular repolarization: key role for β-adrenergic receptor stimulation. Circulation 107: 2753–2760.
View Article
Google Scholar

[409] View Article

[410] Google Scholar

[ref139] 139. Pogwizd SM, Schlotthauer K, Li L, Yuan W, Bers DM (2001) Arrhythmogenesis and contractile dysfunction in heart failure: roles of sodium-calcium exchange, inward rectifier potassium current, and residual β-adrenergic responsiveness. Circ Res 88: 1159–1167.
View Article
Google Scholar

[412] View Article

[413] Google Scholar

[ref140] 140. Yamada KA, Corr PB (1992) Effects of β-adrenergic receptor activation on intracellular calcium and membrane potential in adult cardiac myocytes. J Cardiovasc Electrophysiol 3: 209–224.
View Article
Google Scholar

[415] View Article

[416] Google Scholar

[ref141] 141. MacLennan DH, Kranias EG (2003) Phospholamban: a crucial regulator of cardiac contractility. Nat Rev Mol Cell Biol 4: 566–577.
View Article
Google Scholar

[418] View Article

[419] Google Scholar

[ref142] 142. Eisner D, Bode E, Venetucci L, Trafford A (2013) Calcium flux balance in the heart. J Mol Cell Cardiol 58: 110–117.
View Article
Google Scholar

[421] View Article

[422] Google Scholar

[ref143] 143. Bers DM (2012) Ryanodine receptor S2808 phosphorylation in heart failure. Smoking gun or red herring. Circ Res 110: 796–799.
View Article
Google Scholar

[424] View Article

[425] Google Scholar

[ref144] 144. Marx SO, Reiken S, Hisamatsu Y, Jayaraman T, Burkhoff D, et al. (2000) PKA phosphorylation dissociates FKBP12.6 from the calcium release channel (ryanodine receptor): defective regulation in failing hearts. Cell 101: 365–376.
View Article
Google Scholar

[427] View Article

[428] Google Scholar

[ref145] 145. Zhang H, Makarewich CA, Kubo H, Wang W, Duran JM, et al. (2012) Hyperphosphorylation of the cardiac ryanodine receptor at serine 2808 is not involved in cardiac dysfunction after myocardial infarction. Circ Res 110: 831–840.
View Article
Google Scholar

[430] View Article

[431] Google Scholar

[ref146] 146. Soltis AR, Saucerman JJ (2011) Robustness portraits of diverse biological networks concerved despite order-of-magnitude parameter uncertainty. Bioinformatics 27: 2888–2894.
View Article
Google Scholar

[433] View Article

[434] Google Scholar

[ref147] 147. Rochais F, Abi-Gerges A, Horner K, Lefebvre F, Cooper DMF, et al. (2006) A specific pattern of phosphodiesterases controls the cAMP signals generated by different G_s-coupled receptors in adult rat ventricular myocytes. Circ Res 98: 1081–1088.
View Article
Google Scholar

[436] View Article

[437] Google Scholar

[ref148] 148. Hohl CM, Li Q (1991) Compartmentation of cAMP in adult canine ventricular myocytes: relation to single-cell free Ca²⁺ transients. Circ Res 69: 1369–1379.
View Article
Google Scholar

[439] View Article

[440] Google Scholar

Figures

Abstract

Introduction

Methods

Model Development: Biochemical Part

β1-adrenergic receptor module.

Adenylyl cyclase module.

Phosphodiesterase module.

cAMP-PKA module.

Protein phosphatases and inhibitor-1 module.

cAMP dynamics.

PKA dynamics.

Model Development: Electrophysiological Part

L-type Ca2+ current module.

Fast Na+ current module.

Ryanodine receptor module.

Phospholemman and the Na+-K+ pump module.

Ultra-rapidly activating delayed rectifier K+ current module.

Rapidly recovering transient outward K+ current module.

Time-independent K+ current module.

Phospholamban module.

Troponin I module.

Method of Simulation

Results

cAMP Dynamics During Activation of β1-adrenergic Signaling System: the Effects of Phosphodiesterases

The Effects of Activation of the β1-adrenergic Signaling System on Mouse Action Potential

The Effects of Activation of the β1-adrenergic Signaling System on Ca2+ Dynamics

The Effects of Activation of the β1-adrenergic Signaling System on Na+ Fluxes

The Effects of the Block of Different Populations of ICaL on the Action Potential and [Ca2+]i Transients

Discussion

Compartmentalization of the β1-adrenergic Signaling System

The Effects of the β1-adrenergic Signaling System on Action Potential

The Effects of the β1-adrenergic Signaling System on Ca2+ Dynamics

The Effects of the β1-adrenergic Signaling System on Na+ Fluxes

Model Limitations

Supporting Information

Appendix S1.

Acknowledgments

Author Contributions

References

β₁-adrenergic receptor module.

L-type Ca²⁺ current module.

Fast Na⁺ current module.

Phospholemman and the Na⁺-K⁺ pump module.

Ultra-rapidly activating delayed rectifier K⁺ current module.

Rapidly recovering transient outward K⁺ current module.

Time-independent K⁺ current module.

cAMP Dynamics During Activation of β₁-adrenergic Signaling System: the Effects of Phosphodiesterases

The Effects of Activation of the β₁-adrenergic Signaling System on Mouse Action Potential

The Effects of Activation of the β₁-adrenergic Signaling System on Ca²⁺ Dynamics

The Effects of Activation of the β₁-adrenergic Signaling System on Na⁺ Fluxes

The Effects of the Block of Different Populations of I_CaL on the Action Potential and [Ca²⁺]_i Transients

Compartmentalization of the β₁-adrenergic Signaling System

The Effects of the β₁-adrenergic Signaling System on Action Potential

The Effects of the β₁-adrenergic Signaling System on Ca²⁺ Dynamics

The Effects of the β₁-adrenergic Signaling System on Na⁺ Fluxes