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Research Article

Distinct Redox Regulation in Sub-Cellular Compartments in Response to Various Stress Conditions in Saccharomyces cerevisiae

  • Anita Ayer,

    Affiliation: University of New South Wales, Sydney, Australia

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  • Julia Sanwald,

    Affiliation: University of New South Wales, Sydney, Australia

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  • Bethany A. Pillay,

    Affiliation: University of New South Wales, Sydney, Australia

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  • Andreas J. Meyer,

    Affiliation: INRES-Chemical Signalling, University of Bonn, Bonn, Germany

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  • Gabriel G. Perrone,

    Affiliation: University of Western Sydney, Penrith, Australia

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  • Ian W. Dawes mail

    i.dawes@unsw.edu.au

    Affiliation: University of New South Wales, Sydney, Australia

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  • Published: June 07, 2013
  • DOI: 10.1371/journal.pone.0065240

Abstract

Responses to many growth and stress conditions are assumed to act via changes to the cellular redox status. However, direct measurement of pH-adjusted redox state during growth and stress has never been carried out. Organellar redox state (EGSH) was measured using the fluorescent probes roGFP2 and pHluorin in Saccharomyces cerevisiae. In particular, we investigated changes in organellar redox state in response to various growth and stress conditions to better understand the relationship between redox-, oxidative- and environmental stress response systems. EGSH values of the cytosol, mitochondrial matrix and peroxisome were determined in exponential and stationary phase in various media. These values (−340 to −350 mV) were more reducing than previously reported. Interestingly, sub-cellular redox state remained unchanged when cells were challenged with stresses previously reported to affect redox homeostasis. Only hydrogen peroxide and heat stress significantly altered organellar redox state. Hydrogen peroxide stress altered the redox state of the glutathione disulfide/glutathione couple (GSSG, 2H+/2GSH) and pH. Recovery from moderate hydrogen peroxide stress was most rapid in the cytosol, followed by the mitochondrial matrix, with the peroxisome the least able to recover. Conversely, the bulk of the redox shift observed during heat stress resulted from alterations in pH and not the GSSG, 2H+/2GSH couple. This study presents the first direct measurement of pH-adjusted redox state in sub-cellular compartments during growth and stress conditions. Redox state is distinctly regulated in organelles and data presented challenge the notion that perturbation of redox state is central in the response to many stress conditions.

Introduction

Eukaryotic organisms have evolved to maintain distinct redox environments in organelles, allowing compartmental specific processes to occur. A highly reducing environment is maintained in compartments including the cytosol, mitochondrial matrix and peroxisome to facilitate proper protein folding and activity. Conversely, the endoplasmic reticulum and mitochondrial intermembrane space have been observed to maintain a more oxidizing environment [1], [2]. Aberrant sub-cellular redox environments can be detrimental, affecting a broad range of cellular processes including signal transduction, RNA, DNA and protein synthesis [3][5] and cell cycle regulation [6], [7]. As a result, maintaining appropriate redox homeostasis is critical for cellular function [8]. Redox dysfunction has been implicated in various stress conditions including osmotic, heat and oxidative stress through protein and microarray data, and resistance/sensitivity phenotypes [9][13]. However the exact change to sub-cellular redox state under various stress conditions is unknown.

Cellular redox homeostasis can be significantly affected in cells via mechanisms that alter the state of key redox couples and systems such as the glutathione disulfide/glutathione (GSSG/2GSH) and NADP+/NADPH couples. Additionally, alterations to cellular pH can significantly affect redox homeostasis since many redox reactions are pH dependent [8]. For example, the reduction potential of the GSSG/2GSH couple changes by 59 mV between pH 7 and 8 which alters the effectiveness of glutathione as a redox buffer.

Conventionally, the pH and redox environment of cells have been measured using in vitro assays or dyes. Such methods prohibit the measurement of redox and pH state in an accurate and real-time manner in sub-cellular compartments. The spatiotemporal pattern of intracellular redox and pH changes may differ between cellular compartments especially after stress, and understanding the significance of redox and pH state changes at a compartmental level is extremely important to an understanding of the regulation of these two processes. Development of redox- and pH-responsive fluorescent probes such as roGFP2 [14] and pHluorin [15] have allowed dynamic in vivo analysis of redox state and pH. The sensitivity of these fluorescent proteins was achieved by mutagenesis of wild type green fluorescent protein (GFP). In these GFP variants, changes to redox state or pH alter the structure of GFP leading to alterations in fluorescence emission after excitation at two different wavelengths. By measuring the changes to emission after excitation at 405 nm and 488 nm in cells expressing roGFP2 or pHluorin the redox state and pH of an intracellular compartment can be calculated accurately. As the roGFP2 probes equilibrates predominantly with the GSSG/2GSH couple and is stable between pH 5–8 [16], analyses using targeted roGFP2 and pHluorin probes allow reliable estimation of the sub-cellular state of the glutathione disulfide/glutathione couple adjusted for pH. Unlike in animal cells, roGFP2 in S. cerevisiae responds dynamically to physiological changes in the GSSG/2GSH couple. Consequently, by using organelle-targeted roGFP2/pHluorin constructs in tandem, the contribution of organelles to the overall cellular redox environment under various stress and physiological states can be defined.

Here, we investigated the response of the GSSG/2GSH redox state in Saccharomyces cerevisiae to conditions that have previously been linked to redox dysfunction. Specifically, these analyses were carried out on a compartmental level, investigating the cytosol, mitochondrial matrix and peroxisome using roGFP2 and pHluorin constructs genetically targeted at these organelles. Organellar redox state was determined under various physiological states, with redox state significantly affected by growth phase and carbon source. The sub-cellular redox state was also determined when cells were challenged with common environmental stresses. Both hydrogen peroxide and heat shock significantly altered sub-cellular redox state via two different mechanisms while osmotic stress and exposure to superoxide generators did not alter redox state, highlighting the need to understand the relationship between stress conditions and sub-cellular redox state.

Materials and Methods

Yeast Strains and Growth Medium

S. cerevisiae strains of the BY4743 background were used for all analyses (EUROSCARF). Cells were either grown in fermentative synthetic complete medium lacking uracil (SCURA; 2% w/v D-glucose, 0.17% yeast nitrogen base lacking ammonium and amino acids (BD Difco, Sydney, NSW) and 0.5% ammonium sulphate) or respiratory synthetic complete medium lacking uracil (SGEURA; 2% w/v glycerol, 1% ethanol, 0.17% yeast nitrogen base lacking ammonium sulphate and amino acids (BD Difco, Sydney, NSW) and 0.5% ammonium sulphate). Both media were supplemented as listed in Table S1. All analyses were carried out in SCURA in exponential phase unless otherwise stated. Exponential phase refers to cell cultures with an A600 = 0.5–1 and stationary phase refers to cell cultures with an A600 = 5–6. For continuous monitoring of cell growth cultures were incubated with shaking at 30°C in a Bioscreen C (Oy Growth Curves AB Ltd).

Plasmids

Details of organelle-targeted roGFP2 constructs pAG416-roGFP2 and pAG416-COX4-roGFP2 are described in [17] and pAG416-roGFP2SKL [18]. For details of roGFP2-SKL localization analyses and calibration see [18].

Organelle-targeted pHluorin probes were constructed using PCR amplification and the Invitrogen Gateway System® (Invitrogen Life Technologies, Carlsbad, CA) in a manner analogous to the construction of the organelle-targeted roGFP2 robes. Briefly, the pH-sensitive green fluorescent protein (pHluorin) open reading frame was amplified using PCR from pCB901YpHc (a kind gift from R. Rao). For pAG416-COX4-pHluorin, pHluorin was PCR amplified and the matrix targeting sequence (codons for amino acids 1–25 of the cytochrome oxidase subunit IV gene COX4) was fused at the N-terminus of pHluorin. For the peroxisomal-targeted pHluorin (pAG416-pHluorin-SKL), the peroxisomal C-terminal targeting sequence encoding seryl-lysyl-leucine was added on to the primer used for amplification. attb1 and attb2 sites were added to primers as appropriate so that the resulting localization signal containing pHluorin sequence was flanked by a 5′ attb1 site and a 3′ attb2 site. The resulting PCR fragments were used for the Gateway BP® clonase® reaction using the destination vector pDonr221 generating the plasmids pDonr221-COX4-pHluorin and pDonr221-pHluorin-SKL. These plasmids were used for the Gateway LR® clonase® reaction using the destination vector pAG416GPD-ccdB [19]. All reactions were carried out according to manufacturer’s instructions. Primers used are given in Table S2.

Localization of pHluorin and Organelle-targeted Derivatives

Correct localization of organelle-targeted pHluorin was confirmed by confocal microscopy. Localization of the pHluorin probes was determined using confocal microscopy. For localization analyses cells were grown and treated as follows: 1) cells expressing cytosolically localized pHluorin were grown in SCURA overnight and analyzed microscopically; 2) cells expressing the matrix-targeted pHluorin (COX4-pHluorin) were grown in SCURA overnight and incubated with DAPI (Sigma Aldrich, St Louis, MO) for 30 min to stain DNA; 3) cells expressing the peroxisomal-targeted pHluorin were grown in SCURA overnight and analyzed microscopically. Cells were examined using an Olympus FV-1000 confocal microscope at a magnification of 100× and Brightfield and fluorescence images. Brightfield, GFP and DAPI were visualized using the 543-, 488-, and 405 nm lasers respectively.

Analysis of Compartmental Redox State (EGSH)

BY4743 cells transformed with the roGFP2 constructs were grown in SCURA for 2 d (30°C; 700 rpm), inoculated in SCURA medium and grown with shaking at 25°C until appropriate cell yield had been reached. For analysis of cells in respiratory medium, cells transformed with the roGFP2 constructs were grown in SCURA for 2 d (30°C; 700 rpm), inoculated in SGEURA medium and grown with shaking at 25°C until appropriate cell yield had been reached. Cells were treated as outlined below and then analyzed using the FACS Canto II (BD Bioscience) instrument equipped with a laser that excites at 405 nm and 488 nm. Emission was detected at 512 nm. The ratio of the emission after excitation at 405 nm to that at 488 nm was then calculated. Cells were also treated for 20 min with 10 mM DTT (Astral Scientific, Sydney, NSW) or 10 mM diamide (Sigma Aldrich, St Louis, MO) to obtain measurements of the fully reduced or oxidized (respectively) forms of the roGFP2 probe that are necessary to calculate EGSH as previously reported [20]. EGSH was then calculated as previously described [17] with 10,000 cells counted for each sample. The pH value obtained using pHluorin was used for calculation of EGSH. Data obtained were analyzed with FlowJo version 7.4 software.

Analysis of Compartmental pH

BY4743 cells transformed with the relevant pHluorin construct were grown in SCURA for 2 d (30°C; 700 rpm), inoculated in SCURA medium and grown with shaking at 25°C until appropriate cell yield had been reached. For analysis of cells in respiratory medium, cells transformed with the pHluorin construct were grown in SCURA for 2 d (30°C; 700 rpm), inoculated in SGEURA medium and grown with shaking at 25°C until appropriate cell yield had been reached. Cells were treated as outlined below and then analyzed using the FACS Canto II (BD Bioscience) as described above. To obtain pH values using the pHluorin probe in each compartment, a standard curve was established to allow estimation of compartmental pH by determining the fluorescence of digitonin-permeabilized cells incubated in buffers with pH values of 5 to 8 [21][23]. For calibration of the cytosolically-, mitochondrial matrix-, and peroxisomal-localized pHluorin, cells were suspended in 0.65 M sorbitol containing 100 mg/ml digitonin (Sigma Aldrich, St. Louis, MO) and incubated for 10 min with shaking (600 rpm; 24°C). Cells were pelleted, washed and resuspended in calibration buffer containing 50 mM 2-(N-morpholino)ethanesulfonic acid (MES; Sigma Aldrich, St. Louis, MO), 50 mM N-(2-hydroxyethyl)piperazine-Ń-(2-ethanes​ulfonicacid) (HEPES; Sigma Aldrich, St. Louis, MO), 50 M KCl (Ajax Lab Chemical, Sydney, NSW), 50 mM NaCl (Ajax Lab Chemical, Sydney, NSW), 0.2 M ammonium acetate (Ajax Lab Chemical, Sydney, NSW), 10 mM NaN3 (Ajax Lab Chemical, Sydney, NSW), 10 mM 2-deoxyglucose (Sigma Aldrich, St. Louis, MO), 75 µM monensin (Sigma Aldrich, St. Louis, MO) and 10 µM nigericin (Sigma Aldrich, St. Louis, MO), titrated to different pH values (6.0–8.0) using NaOH in 0.5 pH unit increments. Calibration curves were plotted using the ratio of fluorescence intensity at 405 nm and 488 nm (after background subtraction) against pH. 10,000 cells were counted for each sample and data obtained were analyzed with FlowJo version 7.4 software.

ß -galactoside Assay

The cellular heat shock response was measured using the HSE2-lacZ and HSE12-lacZ heat shock reporter constructs [24]. The HSE2-LacZ construct contains an E. coli lacZ gene encoding ß-galactosidase under the control of the heat shock factor binding motif and the HSE12-lacZ construct contains an E. coli lacZ gene encoding ß-galactosidase linked to a scrambled, heat -inactive promoter. Cells transformed with these constructs were grown to exponential phase (A600 = ~0.5), harvested and analyzed for beta -galactosidase activity [25]. ß-galactosidase activity was expressed as units of ONPG (O-nitrophenyl-ß-D-galactopyranoside) hydrolyzed (nmol) per minute over total protein (mg). For each condition, three independent transformants were assayed.

Propidium Iodide Staining

Cells were harvested by centrifugation, resuspended in 1 ml phosphate buffered saline (PBS) and stained with propidium iodide (10 µg/ml) for 20 min in the dark, washed twice with PBS, and the level of PI staining analysed by microscopy and flow cytometry. Stained cells were analysed with either a FACS Canto II (BD Bioscience) instrument equipped with a laser that excites at 488 nm and emission was detected at 617 nm using a 556 nm long pass filter an a 585/42 broad pass filter or a Leica fluorescence microscope.

Statistical Analyses

For analysis of significance of cell yield and EGSH data, unpaired t-tests were conducted on samples with p = 0.01. For data discussed in the text, if a significant difference was found, this is indicated by the inclusion of a p-value.

Results

All analyses using roGFP2 and pHluorin were performed using flow cytometry (FACS). For FACS analyses, the mean of the population was used to determine redox state and pH after background fluorescence was subtracted with 10,000 cells counted, with non-fluorescent cells making up less than 20% of the population. A representative dot plot generated from flow cytometry analysis of cells expressing cytosolic roGFP2 is shown in Figure 1. Redox and pH shifts were indicated by an increase in emission (after excitation at 405 nm and a simultaneous decrease in emission after excitation at 488 nm) in the test population relative to the control population. Populations generally had a small standard deviation indicating that redox state and pH were maintained across a narrow range in most cells or growth condition. Thus, the redox potentials and pH values obtained reflected the majority of the cell populations studied.

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Figure 1. Representative dot plot of cells expressing cytosolic roGFP2.

Cells expressing cytosolic roGFP2 were grown to exponential phase (A600~0.5) in SCURA and analyzed by flow cytometry. Dot plot of wild-type cells untreated and treated with oxidant (4 mM hydrogen peroxide). Note the shift in the populations after treatment with hydrogen peroxide towards 405 nm. Dot plots were generated using FlowJo™ software.

doi:10.1371/journal.pone.0065240.g001

The roGFP2 probes targeted to the cytosol and mitochondrial matrix and peroxisome were generated and verified as described previously [17], [18]. Localization of organelle targeted pHluorin constructs was analyzed by confocal microscopy (Figure 2A–B) using established markers. Appropriate localization of pHluorin probes was determined in an analogous manner to roGFP2 analyses. To verify specific localization of mitochondrial matrix-targeted pHluorin to mitochondria, cells were grown overnight in SCURA and stained with the mitochondrial marker 4′,6-diamidino-2-phenylindole (DAPI). Mitochondrial matrix-targeted pHluorin localized with DAPI indicating specific mitochondrial matrix localization (Figure 2A). Specific localization of the pHluorin-SKL construct to the peroxisome was demonstrated using the same technique of Van Roermund et al [23] and Ayer et al [18]. In wild-type cells expressing the pHluorin-SKL construct, a punctate fluorescent pattern consistent with peroxisomal localization was observed. We then expressed pHluorin-SKL in pex5 cells, which are defective in the import of peroxisomal proteins with a peroxisomal targeting signal 1 (PTS1) such as -SKL. In pex5 cells expressing pHluorin-SKL, the punctate fluorescent pattern seen in wild-type cells was abolished (Figure 2B). Instead a cytosolic fluorescent pattern was observed indicating that in the wild type the SKL-tagged constructs were correctly targeted and are imported via the PTS1-mediated import pathway into the peroxisome.

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Figure 2. Confocal microscopy images of yeast cells expressing cytosolic, mitochondrial matrix or peroxisomal pHluorin.

A) Wild type cells were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated into SCURA (A600 = 0.001), grown until exponential phase and examined using an Olympus FV-1000 confocal microscope at a magnification of 100X. B) In cells where mitochondrial DNA was visualized cells were incubated with DAPI for 30 min, washed with sterile water and examined. C) pex5 cells were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated into SCURA (A600 = 0.001), grown to exponential phase (A600 = ~0.5) and examined using an Olympus V-1000 confocal microscope at a magnification of 100X.

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The response of roGFP2 probes to redox state has been calibrated in vitro, its stability over an intracellular pH range of 5–8 has also been established [14], [16] and the responsiveness to in vivo redox state change has been confirmed [18]. pHluorin sensitivity to pH was also verified by the construction of calibration curves after incubation of digitonin-permeabilized cells for 50 minutes in various buffers between pH 6.0–8.0. Calibration curves were plotted using the ratio of fluorescence intensity at 405 nm and 488 nm (after background subtraction) against pH for each targeted construct (Figure 3A). All constructs responded to virtually the same extent after digitonin-treatment and incubation in various pH solutions indicating that pHluorin responded equally in all compartments tested. In each respective condition tested, pH was measured using pHluorin and used to calculate EGSH. To verify that changes in pHluorin were redox-independent, pH was determined in wild-type cells transformed with pHluorin constructs treated with DTT, a strong thiol reductant, or diamide, a strong oxidizer of glutathione. No significant change in pH was observed in any compartment upon treatment with DTT or diamide, indicating that changes to pHluorin are specific to changes in intracellular pH and that the pHluorin probes are redox-independent (Figure 3B).

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Figure 3. Verification of organelle-targeted pHluorin responsiveness to pH changes.

A) pHluorin calibration curves: Cells expressing compartment targeted-pHluorin were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were treated with digitonin (100 µg/ml; 10 min; 600 rpm), resuspended in a sorbitol/digitonin solution and then incubated with calibration buffer adjusted to various pH. Cells were analyzed via flow cytometry with 10,000 cells counted for each sample. Calibration curves are indicated for the cytosol (black line), mitochondrial matrix (grey line) and peroxisome (dashed line). B) Effect of diamide treatment on pH as measured by pHluorin in wild-type cells: cells expressing the compartment-targeted pHluorin probes were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were treated with diamide or DTT (30 min; 600 rpm), and analyzed via flow cytometry.

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Redox State in Sub-cellular Compartments is Differentially Affected by Growth Phase and Carbon Source

It is known that changes in carbon source lead to alterations in macromolecule composition and fluxes of redox intermediates through central metabolic pathways [26]. We therefore decided to examine the effect of carbon source and growth phase on sub-cellular redox state. To investigate if the redox state of the cytosol, mitochondrial matrix and peroxisome were affected by growth phase or carbon source, EGSH and pH values were determined in cells transformed with the appropriate constructs during the two main phases of growth (exponential and stationary phase) in both fermentative (SCURA; glucose) and respiratory (SGEURA; glycerol/ethanol) medium. For cells grown fermentatively, the redox states of the cytosol, mitochondrial matrix and peroxisome were estimated to be highly reducing, with the EGSH between −340 to −350 mV (Table 1).

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Table 1. EGSH and pH of wild type cells grown in fermentative (SD) and respiratory (SGE) medium in exponential and stationary phase.

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Peroxisomal EGSH was not affected by growth phase or carbon source. However, cytosolic and mitochondrial matrix EGSH were. With respect to growth phase, both cytosolic and mitochondrial matrix EGSH became more oxidized by 10–15 mV in stationary phase relative to exponential phase in cells grown in glucose (fermentative conditions). This may be expected since cells grown in glucose will have shifted from fermentation to respiration during the diauxic shift prior to stationary phase. It is likely that under respiratory conditions the EGSH will be more oxidizing, due to increased function of the respiratory chain. This was confirmed since the cytosol and matrix redox state were more oxidizing in exponential phase in cells grown on respiratory medium (SGE; glycerol/ethanol) compared to cells growing on fermentative medium (SD; glucose). Moreover, there was no significant shift in redox state between exponential and stationary-phase cells grown in glycerol/ethanol. These results show that the major physiological component in setting EGSH is whether the cells are respiring or not, not the phase of growth. Most clearly, the cytosol and mitochondrial matrix in cells grown under respiratory conditions (stationary phase or growth during any phase in glycerol/ethanol) showed a 10–15 mV shift to more oxidizing conditions compared to fermentative growth (exponential phase in glucose) indicating the effect of respiration on sub-cellular redox state.

The EGSH values presented are more reducing than previously estimated [2], [27][29]. This resulted from the measured pH values of the cytosol and mitochondrial matrix (pH 7.5 and 7.7 respectively) being more basic than those previously estimated [30]. When wild-type cells were grown to stationary phase in respiratory medium, the pH of the cytosol, mitochondrial matrix and peroxisome decreased by approximately 0.4 pH units compared to the pH of cells grown in fermentative medium indicating a change in both redox state and pH as cells switched to respiration.

Sub-cellular Responses to Hydrogen Peroxide and Paraquat

The transcriptional, proteomic and sensitivity/resistance phenotypes of cells treated with H2O2 and paraquat (which leads to generation in cells of the superoxide anion radical; O2.-) have been extensively studied [9], [31][33] with the functions involved in the responses to, and tolerance of, H2O2 and O2.- well documented. While both agents can be deleterious for growth and cell function, the manner in which these two reactive oxygen species (ROS) generators affect the sub-cellular redox environment is less well understood. Dardalhon et al [34] have studied the effects of H2O2 treatment on cytoplasmic and nuclear redox state using the redox sensitive probe rxYFP. However there has been no direct study of the effects of H2O2 on the redox state of the peroxisome or mitochondrial matrix or of superoxide generators in any compartment.

To test the effects of paraquat on the sub-cellular redox state, cells expressing organelle-targeted roGFP2 and pHluorin were grown to exponential phase, treated with 2 mM paraquat for one hour and analyzed immediately for EGSH and pH. Despite this dose of paraquat leading to increased transcription of Mn superoxide dismutase gene [35], there was no significant change of EGSH or pH in the cytosol, mitochondrial matrix or peroxisome (Table 2). From these data, it is unlikely that paraquat or the resulting superoxide anion radical formation affects pH or the redox state of the glutathione redox couple in wild-type cells. This is supported by fact that deletion of SOD1, the cytosolic superoxide dismutase had no effect on cytosolic or mitochondrial EGSH [18].

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Table 2. EGSH and pH of wild type cells grown in SCURA to exponential phase and treated with various stressors for 1 hour.

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To test how rapidly EGSH changes occurred following hydrogen peroxide treatment, cells treated with 2 mM hydrogen peroxide were analysed at five-minute intervals for 30 minutes. EGSH changes were observed as early as 5 minutes post hydrogen peroxide addition, and this change was maximal as no further EGSH changes were observed during the 30 minute treatment. To further investigate the effects of hydrogen peroxide on sub-cellular EGSH, wild-type cells expressing roGFP2 or pHluorin were treated with various concentration of H2O2 (1–20 mM) for 30 min and redox state and pH analyzed in the cytosol, mitochondrial matrix and peroxisome (Figure 4A–C). All compartments tested followed a similar trend in EGSH upon hydrogen peroxide treatment. The redox state of every compartment tested became more oxidized with increasing doses of hydrogen peroxide. As little as 1 mM H2O2 led to a significant shift of EGSH in all compartments tested (p<0.01), with a ΔEGSH of 40–50 mV after treatment. Treatment with 20 mM hydrogen peroxide shifted the roGFP2 probe near its oxidized limit with a ΔEGSH of ~100 mV after treatment with 20 mM H2O2. While this is a high concentration of H2O2, it does indicate the sensitivity and range of roGFP2 in vivo. Interestingly, treatment with H2O2 affected the pH of each compartment significantly (p<0.01). The pH of the cytosol, mitochondrial matrix and peroxisome all decreased by approximately 1 pH unit after 30 minutes of H2O2 treatment and this pH shift contributed significantly to the observed changes in redox state changes.

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Figure 4. Effect of hydrogen peroxide on compartmental EGSH and pH.

A-C) Cells were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were then treated with various doses of hydrogen peroxide for 30 min and pH and redox environment analyzed. (A cytosolic pH and EGSH, B) mitochondrial matrix pH and EGSH, C) peroxisomal pH and EGSH. 10,000 cells were counted for each sample. Each experiment was conducted in triplicate with error bars representing the standard deviation of three experiments. Error bars may be difficult to visualise as the errors are in the ~5 mV range.

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An important aspect in the physiology of cells under stress is the manner in which they recover, with the kinetics of recovery a good indicator of the mechanisms involved. In order to study the recovery of cells after exposure to H2O2, cells were treated with 2 mM H2O2 for 30 minutes, washed and re-suspended in fresh medium and the redox state and pH measured every two minutes. The 2 mM H2O2 dose was chosen since this concentration led to oxidation of half of the roGFP2 probe as determined in previous H2O2 experiments and led to a significant shift in EGSH without causing cell death (Figure 4A–C). In response to H2O2 treatment (2 mM; 30 min), the cytosol, mitochondrial matrix and peroxisome displayed distinct kinetics of response and recovery (Figure 5A–C). All compartments became more oxidizing by approximately 30 to 40 mV and more acidic by 1 pH unit. In the 40 minute period studied, the EGSH and pH in the cytosol and mitochondrial matrix recovered by 80–90%, with the cytosol recovering most rapidly, within four minutes of cells being re-suspended in fresh medium. The mitochondrial matrix exhibited slightly slower kinetics of recovery, with changes in EGSH and pH observed 10 minutes after transfer to fresh medium. However, the peroxisome was the most severely affected compartment in terms of redox state and pH recovery. Following an initial recovery after 10 minutes in fresh medium the EGSH in the peroxisome reached a plateau, with the EGSH recovering only ~25% of the change after hydrogen peroxide exposure. In the same way, in the time period studied, the pH of the peroxisome was only able to recover by 0.2 pH units and did not return to that of untreated cells. These results indicate that there are specific and individual responses in different organelles to hydrogen peroxide. Importantly, the data highlight that there is distinct spatiotemporal regulation of redox state.

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Figure 5. Dynamic recovery of cells after hydrogen peroxide treatment.

Cells were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Starting EGSH was measured then cells were treated with hydrogen peroxide (2 mM; 20 min; 25°C), washed and resuspended in fresh medium, and pH and redox state analyzed by flow cytometry at two-minute intervals. A) cytosolic pH and EGSH, B) mitochondrial matrix pH and EGSH and C) peroxisomal pH and EGSH. 10,000 cells were counted for each sample. Each experiment was conducted in triplicate with error bars representing the standard deviation of three experiments. The EGSH and pH in untreated (control cells) is indicated by the marked dashed lines. Some error bars may be difficult to visualise as the errors are in the ~5 mV range.

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In order to put these redox changes in the context of the effects of the 2 mM H2O2 treatment on the survival and growth of the cultures, cell survival in terms of ability of cells to replicate after treatment was assessed by plate counts before and after treatment, and the effects on population growth was determined by continuous monitoring of the growth of untreated and treated cultures. After treatment with 2 mM H2O2 for 30 minutes 77% of the wild-type cells survived to be able to produce a colony. The growth curves for the treated and untreated cells are given in Figure S1A. The untreated culture showed no lag phase, while the population of treated cells had a lag of 139 minutes (uncorrected for cells that are not going to replicate). The doubling time was 130 minutes, hence the correction for 77% survival would be 48 minutes for the cells to grow to the starting OD. The lag phase for the overall population after 2 mM treatment was therefore about 90 minutes. This indicates that the population of H2O2-treated cells takes about 90 minutes to recover full growth rate, which is longer than the time it takes for the population to recover the cytoplasmic and mitochondrial redox potentials. Some cells may recover earlier given the sigmoidal nature of the growth curve, although there was little increase in growth of the treated culture in the first 45 minutes after the treatment. These data indicate that cells recover their cytoplasmic and mitochondrial EGSH before they resume growth at a normal rate, but this need not imply a causal relationship between redox recovery and delay in growth.

Compartmental Redox State in Response to Heat Induced Stress

Many chemical and environmental stress conditions trigger comparable transcriptional responses and the common component of these has been termed the environmental stress response (ESR) [9]. An important feature of the environmental stress response is up-regulation of systems for the detoxification of reactive oxygen species indicating that oxidative stress may be an important component in the response of cells to a wide variety of stress conditions. For heat stress in particular this view has led to the theory that oxidative stress is a component of the response to heat-stress [36], [37]. To investigate the effect of heat shock on compartmental redox state and pH, cells separately transformed with the roGFP2 and pHluorin constructs were grown to exponential phase and subjected to thermal shock by shifting them from 25°C to 42°C for 60 min. Redox state and pH were then measured and EGSH calculated. This heat shock regime led to a 275-fold induction of the heat shock response as measured using a heat-shock element lacZ reporter HSE2-lacZ [24] (Figure 6A). The HSE2-lacZ construct is an artificial heat-shock promoter coupled to the lacZ gene, which is induced under conditions of heat stress leading to production of ß-galactosidase. Increased ß-galactosidase activity correlates with increased conditions of cellular heat stress.

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Figure 6. Effect of heat shock on compartmental EGSH and pH.

A) Wild-type cells with the HSE2-lacZ (heat-shock response induction reporter) construct were pregrown in SCURA (48 h; 30°C; 600 rpm) and then inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were then shifted to 42°C for 60 min and harvested. β-galactosidase and total protein (Bradford) assays were carried out on cell pellets and specific activity determined. B-C) Cells were pregrown in SCURA (48 h; 30°C; 600 rpm), inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were then shifted to 42°C for 60 min and EGSH B) and pH C) analyzed via flow cytometry. 10,000 cells were counted for each condition. Each experiment was conducted in triplicate with error bars representing the standard deviation of three experiments.

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EGSH in all compartments tested became significantly more oxidized by the temperature shift from 25°C to 42°C (p<0.01), with a 40 mV decrease in EGSH observed after 60 minutes at 42°C in all compartments (Figure 6B). Interestingly, intracellular pH was significantly affected by heat shock (Figure 6B). Heat shock resulted in every compartment tested becoming significantly more acidic (p<0.01) and this shift in intracellular pH modulated the large change in EGSH rather than direct changes to the glutathione couple since the roGFP2 R405/488 ratio did not undergo a major change. A recent screen (Jarolim S and Dawes IW, unpublished data) has also identified numerous genes required for vacuolar H+-ATPase activity to be essential for survival to heat stress. Since the H+-ATPase functions to pump protons from the cell, this highlights the importance of cellular functions restoring pH homeostasis as central in the cellular response to heat stress. Significantly, these data highlight a stress condition that can mediate changes in redox state, primarily through changes in intracellular pH rather than through directly disturbance of a redox couple(s).

Compartmental Redox State in Response to Sorbitol, Sodium and Potassium Induced Stress

To determine if other stresses affected redox homeostasis, we analyzed the redox state of the cytosol, mitochondrial matrix and peroxisome in wild-type cells after exposure to hyperosmotic or salt-induced stress. Wild-type cells transformed with roGFP2 or pHluorin constructs were grown to exponential phase and treated with 1.8 M sorbitol, or 0.9 M NaCl or 1.3 M KCl for 60 minutes. Redox state and pH were then measured and EGSH calculated. All concentrations and times chosen have been reported to induce known osmotic shock-responsive pathways and indicators of stress such as P-bodies [10], [38]. Treatment with sorbitol, NaCl and KCl did not significantly affect the redox state or pH of the cytosol, mitochondrial matrix or peroxisome (Table 2). Results indicate that while sorbitol-, sodium-, and potassium-induced stress may lead to the up-regulation of some oxidative stress-response genes [9], [10], [38], [39], these stresses do not directly affect the sub-cellular redox state measured using roGFP2.

Redox State and Hydrogen Peroxide-mediated Adaptation

Cells pre-treated with a low sub-lethal level of stress have an increased ability to survive subsequent challenge [31], [40]. Cellular adaptation has been observed in response to numerous ROS or ROS-generating agents such as H2O2 [31], menadione [40], [41] and linoleic acid hydroperoxide [42]. While the effect of adaptation to H2O2 on survival has been well studied [43], the effect of the adaptation process on organelles and redox state is unknown. To investigate whether redox changes may be involved in the adaptive process, wild-type cells expressing roGFP2 or pHluorin were treated with a low adaptive dose of H2O2 (0.2 mM) for one hour and subsequently challenged with 2 mM H2O2 for 30 minutes. Redox state and pH were then calculated (Table 3). As in previous experiments, 2 mM H2O2 was chosen since it significantly affected EGSH in all compartments tested and this dose has been used previously to examine how adaptation affects survivability [31]. 0.2 mM hydrogen peroxide concentration was chosen as an adaptive dose using the adaptation data from Ng et al [43]. Additionally, cells treated with 0.2 mM hydrogen peroxide did not show a shift in EGSH during 60 minutes treatment. As controls, cells were treated with each H2O2 concentration (0.2 mM or 2 mM) individually to ascertain the effects of each on redox state and pH. Only a slight change in EGSH was observed in cells treated with the adaptive dose of H2O2 (0.2 mM), indicating that changes in EGSH are not likely to be the trigger for an adaptive response. Treatment with 2 mM H2O2 led to a large and significant decrease in EGSH (70 mV). However, EGSH in all compartments remained approximately ~10 mV higher in cells pretreated with 0.2 mM H2O2 and subsequently challenged with 2 mM H2O2 as opposed to cells that were only exposed to 2 mM H2O2. This difference in EGSH (10–12 mV) in each compartment) was statistically significant, and hence EGSH might be involved in the later stages of an adaptive response.

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Table 3. EGSH and pH of wild type, yap1 and skn7 cells grown in SCURA to exponential phase and during the adaptive response to hydrogen peroxide treatment.

doi:10.1371/journal.pone.0065240.t003

Both the Yap1p and Skn7p transcription factors are key mediators of resistance to H2O2 and the YAP1 and SKN7 genes are required for a maximal adaptive response [43]. Additionally, both YAP1 and SKN7 have been identified as essential for the maintenance of cytosolic, mitochondrial matrix and peroxisomal redox state, indicating that both transcription factors sit at the boundary of maintenance-response systems [18]. From these data it has been concluded that expression of some genes regulated by Yap1p and Skn7p are important for steady-state redox homeostasis, while induction and activation of target genes appears important for mounting appropriate responses to oxidative stress [18]. If the redox state changes observed in the wild type after adaption with a low adaptive hydrogen peroxide dose are part of the adaptive process once the transcription factors are activated, the redox changes would not be observed in the yap1 or skn7 mutants. Hence, yap1 and skn7 mutants were treated as per the wild type and redox state and pH in the cytosol, mitochondrial matrix and peroxisome were determined (Table 3).

The data in Table 3 indicate that the yap1 and skn7 mutants both had significantly higher cytosolic EGSH than the wild type (by 30 mV) and mitochondrial matrix EGSH (by 20 mV), but there was much less difference in the peroxisomal EGSH. Previous studies with whole cells have shown that deletion of YAP1 or SKN7 does affect the redox state of the glutathione couple [27], [43], the present data indicate that redox homeostasis is affected by these deletions to a greater degree in the cytosol than the mitochondrial matrix and is little affected in the peroxisome for which there may be different systems responsible for maintenance of redox status.

There was very little change slight in redox state in all compartments tested in both the yap1 and skn7 mutants after treatment with 0.2 mM H2O2 as was found for the wild type (Table 3). Treatment with 2 mM H2O2 resulted in a decrease in cytoplasmic EGSH by 70 mV for the wild type (to −280 mV), 55 mV (to −265 mV) for yap1 cells and 40 mV (to −279 mV) in skn7 cells. There were similar changes in the other two compartments, and interestingly the EGSH in each compartment in treated cells of the wild type and mutants was around −280 mV (with the exception of the cytoplasm in the yap1 mutant. This indicates that H2O2 treatment affects all compartments in the cell to almost the same extent regardless of whether the cell was initially in a more oxidised state due to the yap1 or skn7 mutation. This may reflect the extent of oxidation of glutathione by the oxidant.

In parallel with the wild type, EGSH in all compartments remained approximately ~10 mV higher in the yap1 and skn7 cells pretreated with 0.2 mM H2O2 and subsequently challenged with 2 mM H2O2 compared to cells that were only treated with 2 mM H2O2. Given that Yap1p and Skn7p have been shown to be key mediators in the adaptive process [43], and the responses of cells observed were comparable to those in the wild type, it is unlikely that redox state changes per se are important subsequent events in the cellular adaptation to H2O2. As an additional control, wild type, yap1 and skn7 cells were stained with propidium iodide directly after each hydrogen peroxide treatment to assess cell vitality and to assess the level of dead cells in the cell populations that were assessed by FACS. All cells stained had very low levels of PI staining following any hydrogen peroxide treatment indicating that there was a low level of dead cells analysed in the roGFP2 and pH analyses (Figure S2). These analyses were performed by microscopy and flow cytometry with identical results. There were, however, differences in the colony-forming ability of the wild-type (77%), yap1 (63%) and skn7 (35%) cells after treatment with 2 mM H2O2, indicating that while the cells maintained membrane integrity after treatment there were differences in their longer term survival. Furthermore, directly after each hydrogen peroxide treatment, wild-type, yap1 and skn7 cells were diluted to OD600 0.05 and growth was measured continuously to establish if any of the treatments affected cell growth. All strains showed a lag in growth following treatment with 2 mM H2O2 or the combined adaptive 0.2 mM followed by 2 mM treatment, as discussed above for the wild type, and these lags were comparable between the wild type and mutants (Figure S1B–D).

Discussion

A key limitation in redox biology has been the ability to measure the status of key redox couples at the sub-cellular level. The advent of genetically encoded fluorescent probes such as roGFP2 and pHluorin has allowed compartmental redox dynamics to be studied in an in-depth manner for the first time. While redox and pH sensors have been targeted to various organelles [14], [30], [44], [45], this is the first study to utilise a redox and pH sensor in tandem to specifically monitor the sub-cellular GSSG/2GSH redox couple during various physiological states and stress conditions. By using roGFP2 and pHluorin localized to the cytosol, mitochondrial matrix and peroxisome, a better understanding can be gained of the precise nature of sub-cellular redox homeostasis during changing cellular settings especially during stress conditions.

The EGSH values obtained for the cytosol, mitochondrial matrix and peroxisome in this study are more reducing than previously calculated [27]. Using a whole-cell method, Drakulic and colleagues estimated the EGSH of wild-type cells to be approximately −230 mV, which is ~100 mV more positive than the EGSH values reported here. The difference can be explained by analyses provided by roGFP2 and pHluorin being compartment-specific rather than ‘whole-cell’ as in previous studies and that an assumed cellular pH of 7 was used previously when calculating redox state. Use of another redox-sensitive fluorescent probe rxYFP has estimated cytosolic EGSH to be −274 mV [29] and −286 mV [2] and mitochondrial matrix EGSH to be - 296 mV [2] in wild-type cells. While these values are significantly more reducing than the previous whole-cell estimates, they are still considerably different to the values obtained in this study since compartmental pH was not measured. In the present study the pH in both the cytosol and mitochondrial matrix was found to be slightly more basic by 0.2–0.3 pH units than previously estimated in S. cerevisiae using less specific, whole-cell methods. Previous values for the pH of the cytosol and mitochondrial matrix have ranged from pH 7–7.2 [23], [30] and pH 7.2–7.5 [30] respectively. The outcome of a more basic sub-cellular pH is significant, leading to a more reducing redox environment based on the GSSG/2GSH couple.

The standard half-cell reduction potential of the glutathione couple is −240 mV [8], however a wild-type EGSH value of approximately −340 mV was obtained in the three compartments tested. This puts the cellular redox state closer to that of the NADP+/NADPH and NAD+/NADH couples which have half-cell reduction potentials of −315 mV [46], [47] and −316 mV [8], [47] respectively. It may appear unfavourable for NADPH to reduce GSSG to GSH since the NADP+/NADPH couple has an E0′ value of −315 mV while the EGSH of the cellular compartments tested here was approximately −340 mV. However the concentration of redox species must be taken into account when determining the intracellular half-cell redox potential of any redox couple [8]. Using an NADP+/NADPH ratio of 100:1 [48] the ENADPH is −374 mV. The highly reducing nature of the cytosol, mitochondrial matrix and peroxisome also reflects the critical role of NADPH in providing the primary source of reducing equivalents for the glutathione couple, with the need to maintain a high NADPH:NADP+ ratio driving the glutathione couple and to maintain redox buffering.

A central question in redox biology is whether compartments have distinct redox regulation and the possible crosstalk that may exist between organelles in the overall maintenance of cellular redox homeostasis. Despite all organelles tested being highly reducing and slightly alkaline, there were differences in steady state EGSH and pH between all compartments. Following H2O2 challenge sub-cellular compartments respond distinctly - the cytosol, mitochondrial matrix and peroxisome all responded and recovered differently after treatment with 2 mM H2O2 for 20 min. It is highly probable that the distinct nature of the response and recovery of sub-cellular redox environments to redox state change is a reflection of the redox buffering and antioxidant capabilities of each compartment. The peroxisome in S. cerevisiae is known to only contain three antioxidant-related enzymes, a catalase, a NADP+-dependent isocitrate dehydrogenase and an omega-class glutathione transferase encoded by CTA1 [49][51], IDP3 [52] and GTO1 [51] respectively. The lack of multiple systems for restoring redox state may explain the failure of peroxisomes to re-equilibrate the GSSG/2GSH couple in the time studied. This highlights the importance of studying sub-cellular compartments individually rather than viewing the cell as having a singular redox environment.

Overall these data favour the idea that changes in antioxidant enzymes or redox–related genes observed through transcriptomic or phenotypic analyses should not be used to extrapolate to changes to cellular or sub-cellular redox state. Out of all the stresses tested in this study, only two (H2O2 and heat stress) were found to alter sub-cellular redox state despite all stresses being previously associated with redox dysfunction. Interestingly, H2O2 and heat stress modulated changes to EGSH in different ways. Under H2O2 stress both the GSSG/2GSH couple and pH changed, contributing to the overall change in EGSH. Conversely, after heat stress there was little change observed in the GSSG/2GSH couple despite reports of decreased thermotolerance in cells mutated in key antioxidant enzymes [37], [53]. The changes to intracellular pH observed were large enough to alter the intracellular redox state significantly in the cytosol, mitochondrial matrix and peroxisome. These data highlight the role of pH in redox buffering systems, and pH homeostasis in cells is an important component to study when attempting to identify mechanisms affecting redox state changes. It is possible that there are stresses that have not been conventionally linked with redox dysfunction that do perturb redox state through intracellular pH changes.

The data also raises some interesting questions about how intracellular redox state is viewed. In cells there exist multiple redox couples that are important and relatively independent thermodynamically, with varying kinetic interactions including the thioredoxin couple and protein thiols. While roGFP2 provides an excellent read-out of the GSSG/2GSH couple, the stresses tested may affect other redox couples significantly. For example, paraquat generates the superoxide anion radical that is deleterious to the cell, yet paraquat-treated cells did not exhibit a change in the glutathione couple measured by roGFP2. It is likely that paraquat treatment and subsequent superoxide anion radical formation affect cellular redox homeostasis in some manner, but the data presented here indicated that is unlikely that this directly involves the GSSG/2GSH couple. Examples such as these highlight the need for specificity when discussing the redox environment and redox dysfunction. The stresses tested in this study were stress conditions that have been conventionally associated with redox state changes. However, glutathione homeostasis is also important in iron metabolism [17]; [54], iron-sulfur transport and in the detoxification of reactive electrophiles such as heavy metals and xenobiotics. Furthermore, processes that affect iron metabolism (such as iron starvation) or the level of reactive electrophiles present in cells may in turn alter compartmental glutathione concentrations conditions. It would be of interest to test these stresses to understand their effect on compartmental redox state based on the glutathione couple.

There have been many studies investigating the molecular mechanisms underpinning the ability of cells to adapt to various stress conditions. In the study of Ng et al (2008) [43], yap1 and skn7 mutants were identified as having a much reduced but still detectable ability to adapt to H2O2. Given the importance of Yap1p and Skn7p in redox homeostasis, it was hypothesized that a component of the adaptive response is dependent on the expression of genes important for redox regulation, with a resetting of redox homeostasis required for adaptation. However, the results of this current study indicate that during adaption to H2O2, redox homeostasis can occur independently of the Yap1/Skn7 transcription factors. The resistance to changes in EGSH brought about by 0.2 mM H2O2 pre-treatment may reflect the basal level of adaptive ability that yap1 and skn7 cells can undergo but this level is not enough to change the level of survival after H2O2 treatment.

The parallel analyses of cytosolic, mitochondrial matrix and peroxisomal redox states using roGFP2 and pHluorin carried out in this study have allowed for the monitoring of distinct glutathione redox changes under various conditions. It is clear that changes in sub-cellular redox state occur in a distinct manner in response to stress, with each organelle a discrete redox unit. Data from Dardalhon et al [34] also exemplifies this, since they show that the cytosolic and nuclear redox states are to some extent regulated independently, with both the thioredoxin and glutathione systems important. There is also some conflicting data indicating that the redox state of the mitochondrial inter-membrane space (IMS) may be regulated independently from the cytosol and mitochondrial matrix [2], [17], [55] - the variation in reported IMS EGSH values may possibly be due to strain background differences. The data presented in this study reinforce that sub-cellular redox state can be affected through alterations to the glutathione couple, pH or both. In particular the data reinforces the idea that changes to indicators of oxidative stress such as antioxidant enzymes do not always accurately reflect changes in the sub-cellular redox environment and challenges current ideas around the role of cellular redox status in stress responses.

Supporting Information

Figure S1.

Cell growth of WT, yap1 and skn7 cells after various hydrogen peroxide treatments: Cells were pregrown in SCURA (48 h; 30°C; 600 rpm) inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were left untreated or treated with hydrogen peroxide (0.2 mM for 60 min OR 2 mM for 30 min; OR 0.2 mM for 60 min followed by 2 mM for 30 min; 25°C). After hydrogen peroxide treatment, cells were diluted to OD600 = 0.05 and OD600 was measured every 15 min using a Bioscreen C.

doi:10.1371/journal.pone.0065240.s001

(TIF)

Figure S2.

Propidium iodide staining of WT, yap1 and skn7 cells after various hydrogen peroxide treatments: Cells were pregrown in SCURA (48 h; 30°C; 600 rpm) and then inoculated in SCURA (A600 = 0.001) and grown (25°C; 600 rpm) until exponential phase (A600 = ~0.5). Cells were harvested by centrifugation, resuspended in phosphate buffered saline (PBS), stained with propidium iodide (10 ug/ml) in the dark for 20 min. Cells were washed twice with PBS and level of PI staining analysed by microscopy and flow cytometry. Cells were left untreated or treated with hydrogen peroxide (0.2 mM for 60 min OR 2 mM for 30 min; OR 0.2 mM for 60 min followed by 2 mM for 30 min; 25°C). After hydrogen peroxide treatment the level of PI staining was analysed by microscopy and flow cytometry.

doi:10.1371/journal.pone.0065240.s002

(TIF)

Table S1.

Supplements for synthetic complete (SC) medium.

doi:10.1371/journal.pone.0065240.s003

(DOC)

Table S2.

Primers used in generation of mitochondrial matrix and peroxisomal targeted pHluorin probes.

doi:10.1371/journal.pone.0065240.s004

(DOCX)

Author Contributions

Conceived and designed the experiments: IWD AA GGP. Performed the experiments: AA JS BAP. Analyzed the data: AA JS IWD GGP. Contributed reagents/materials/analysis tools: IWD AJM GGP. Wrote the paper: AA IWD GGP.

References

  1. 1. Hwang C, Sinskey AJ, Lodish HF (1992) Oxidized redox state of glutathione in the endoplasmic reticulum. Science 257: 1496–1502.
  2. 2. Hu J, Dong L, Outten CE (2008) The redox environment in the mitochondrial intermembrane space is maintained separately from the cytosol and matrix. J Biol Chem 283: 29126–29134.
  3. 3. Zehavi-Willner T, Kosower EM, Hunt T, Kosower NS (1971) Glutathione. V. The effects of the thiol-oxidizing agent diamide on initiation and translation in rabbit reticulocytes. Biochim Biophys Acta 228: 245–251.
  4. 4. Zehavi-Willner T (1973) The possible role of glutathione in protein biosynthesis. Isr J Med Sci 9: 129–135.
  5. 5. Matthews JR, Wakasugi N, Virelizier JL, Yodoi J, Hay RT (1992) Thioredoxin regulates the DNA binding activity of NF-kappa B by reduction of a disulphide bond involving cysteine 62. Nucleic Acids Res 20: 3821–3830.
  6. 6. Shackelford RE, Kaufmann WK, Paules RS (2000) Oxidative stress and cell cycle checkpoint function. Free Radic Biol Med 28: 1387–1404.
  7. 7. Burhans WC, Heintz NH (2009) The cell cycle is a redox cycle: linking phase-specific targets to cell fate. Free Radic Biol Med 47: 1282–1293.
  8. 8. Schafer FQ, Buettner GR (2001) Redox environment of the cell as viewed through the redox state of the glutathione disulfide/glutathione couple. Free Radic Biol Med 30: 1191–1212.
  9. 9. Gasch AP, Spellman PT, Kao CM, Carmel-Harel O, Eisen MB, et al. (2000) Genomic expression programs in the response of yeast cells to environmental changes. Mol Biol Cell 11: 4241–4257.
  10. 10. Rep M, Krantz M, Thevelein JM, Hohmann S (2000) The transcriptional response of Saccharomyces cerevisiae to osmotic shock. J Biol Chem 275: 8290–8300.
  11. 11. Causton HC, Ren B, Koh SS, Harbison CT, Kanin E, et al. (2001) Remodeling of yeast genome expression in response to environmental changes. Mol Biol Cell 12: 323–337.
  12. 12. Thorpe GW, Fong CS, Alic N, Higgins VJ, Dawes IW (2004) Cells have distinct mechanisms to maintain protection against different reactive oxygen species: oxidative-stress-response genes. Proc Natl Acad Sci USA 101: 6564–6569.
  13. 13. Tucker CL, Fields S (2004) Quantitative genome-wide analysis of yeast deletion strain sensitivities to oxidative and chemical stress. Comp Func Genom 5: 216–224.
  14. 14. Hanson GT, Aggeler R, Oglesbee D, Cannon M, Capaldi RA, et al. (2004) Investigating mitochondrial redox potential with redox-sensitive green fluorescent protein indicators. J Biol Chem 279: 13044–13053.
  15. 15. Miesenbock G, De Angelis DA, Rothman JE (1998) Visualizing secretion and synaptic transmission with pH-sensitive green fluorescent proteins. Nature 394: 192–195.
  16. 16. Gutscher M, Pauleau AL, Marty L, Brach T, Wabnitz GH, Samstag Y, Meyer AJ, Dick TP (2008) Real-time imaging of the intracellular glutathione redox potential. Nat Meth 5: 553–559.
  17. 17. Ayer A, Tan SX, Grant CM, Meyer AJ, Dawes IW (2010) The critical role of glutathione in maintenance of the mitochondrial genome. Free Radic Biol Med 49: 1956–1968.
  18. 18. Ayer A, Fellermeier S, Fife C, Li SS, Smits G, Meyer AJ, Dawes IW, Perrone GG (2012) A genome-wide screen in yeast identifies specific oxidative stress genes required for the maintenance of sub-cellular redox homeostasis. PLoS ONE 7:(9) e447278.
  19. 19. Alberti S, Gitler AD, Lindquist S (2007) A suite of Gateway cloning vectors for high throughput genetic analysis in Saccharomyces cerevisiae. Yeast 24: 913–919.
  20. 20. Schwarzlander M, Fricker MD, Muller C, Marty L, Brach T, et al. (2008) Confocal imaging of glutathione redox potential in living plant cells. J Microsc 231: 299–316.
  21. 21. Brett CL, Tukaye DN, Mukherjee S, Rao R (2005) The yeast endosomal Na+ (K+)/H+ exchanger Nhx1 regulates cellular pH to control vesicle trafficking. Mol Biol Cell 16: 1396–1405.
  22. 22. Ali R, Brett CL, Mukherjee S, Rao R (2004) Inhibition of sodium/proton exchange by a Rab-GTPase-activating protein regulates endosomal traffic in yeast. J Biol Chem 279: 4498.
  23. 23. van Roermund CWT, de Jong M, IJlst L, van Marle J, Dansen TB, et al. (2004) The peroxisomal lumen in Saccharomyces cerevisiae is alkaline. J Cell Sci 117: 4231–4237.
  24. 24. Sorger PK, Pelham HR (1987) Purification and characterization of a heat-shock element binding protein from yeast. EMBO J 6: 3035–3041.
  25. 25. Rose M, Botstein D (1983) [9] Construction and use of gene fusions to lacZ ([beta]-galactosidase) that are expressed in yeast. Meth Enzym 101: 167–180.
  26. 26. Cortassa S, Aon JC, Aon MA (1995) Fluxes of carbon, phosphorylation, and redox intermediates during growth of Saccharomyces cerevisiae on different carbon sources. Biotech Bioengin 47: 193–208.
  27. 27. Drakulic T, Temple MD, Guido R, Jarolim S, Breitenbach M, et al. (2005) Involvement of oxidative stress response genes in redox homeostasis, the level of reactive oxygen species, and ageing in Saccharomyces cerevisiae. FEMS Yeast Res 5: 1215–1228.
  28. 28. Björnberg O, Østergaard H, Winther JR (2006) Measuring intracellular redox conditions using GFP-based sensors. Antiox Redox Signal 8: 354–361.
  29. 29. Lopez-Mirabal HR, Winther JR (2008) Redox characteristics of the eukaryotic cytosol. Biochim Biophys Acta-Molecular Cell Research 1783: 629–640.
  30. 30. Orij R, Postmus J, Ter Beek A, Brul S, Smits GJ (2009) In vivo measurement of cytosolic and mitochondrial pH using a pH-sensitive GFP derivative in Saccharomyces cerevisiae reveals a relation between intracellular pH and growth. Microbiol 155: 268–278.
  31. 31. Collinson LP, Dawes IW (1992) Inducibility of the response of yeast cells to peroxide stress. J Gen Microbiol 138: 329–335.
  32. 32. Lee FJ, Hassan HM (1985) Biosynthesis of superoxide dismutase in Sacchromyces cerevisiae: Effects of paraquat and copper. J Free Radic Biol Med 1: 319–325.
  33. 33. Outten CE, Falk RL, Culotta VC (2005) Cellular factors required for protection from hyperoxia toxicity in Saccharomyces cerevisiae. Biochemical J 388: 93–101.
  34. 34. Dardalhon M, Kumar C, Iraqui I, Vernis L, Kienda G, et al. (2012) Redox-sensitive YFP sensors monitor dynamic nuclear and cytosolic glutathione redox changes. Free Radic Biol Med 52: 2254–2265.
  35. 35. Galiazzo F, Labbe-Bois R (1993) Regulation of Cu, Zn-and Mn-superoxide dismutase transcription in Saccharomyces cerevisiae.. FEBS Letts 315: 197–200.
  36. 36. Davidson JF, Whyte B, Bissinger PH, Schiestl RH (1996) Oxidative stress is involved in heat-induced cell death in Saccharomyces cerevisiae. Proc Natl Acad Sci USA 93: 5116–5121.
  37. 37. Sugiyama K, Izawa S, Inoue Y (2000) The Yap1p-dependent induction of glutathione synthesis in heat shock response of Saccharomyces cerevisiae. J Biol Chem 275: 15535–15540.
  38. 38. Romero-Santacreu L, Moreno J, PÈrez-OrtÌn JE, Alepuz P (2009) Specific and global regulation of mRNA stability during osmotic stress in Saccharomyces cerevisiae.. RNA 15: 1110–1120.
  39. 39. Posas F, Chambers JR, Heyman JA, Hoeffler JP, de Nadal E, et al. (2000) The transcriptional response of yeast to saline stress. J Biol Chem 275: 17249–17255.
  40. 40. Flattery-O’Brien J, Collinson LP, Dawes IW (1993) Saccharomyces cerevisiae has an inducible response to menadione which differs from that to hydrogen peroxide. J Gen Microbiol 139: 501–507.
  41. 41. Jamieson DJ (1992) Saccharomyces cerevisiae has distinct adaptive responses to both hydrogen peroxide and menadione. J Bact 174: 6678–6681.
  42. 42. Evans MV, Turton HE, Grant CM, Dawes IW (1998) Toxicity of linoleic acid hydroperoxide to Saccharomyces cerevisiae: involvement of a respiration-related process for maximal sensitivity and adaptive response. J Bact 180: 483–490.
  43. 43. Ng CH, Tan SX, Perrone GG, Thorpe GW, Higgins VJ, et al. (2008) Adaptation to hydrogen peroxide in Saccharomyces cerevisiae: the role of NADPH-generating systems and the SKN7 transcription factor. Free Radic Biol Med 44: 1131–1145.
  44. 44. van Lith M, Tiwari S, Pediani J, Milligan G, Bulleid NJ (2011) Real-time monitoring of redox changes in the mammalian endoplasmic reticulum. J Cell Sci 124: 2349–2356.
  45. 45. Yano T, Oku M, Akeyama N, Itoyama A, Yurimoto H, et al. (2010) A novel fluorescent sensor protein for visualization of redox states in the cytoplasm and in peroxisomes. Mol Cell Biol 30: 3758–3766.
  46. 46. Jensen MA, Elving PJ (1984) Nicotinamide adenine dinucleotide (NAD+). Formal potential of the NAD+/NAD couple and NAD dimerization rate. Biochim Biophys Acta -Bioenergetics 764: 310–315.
  47. 47. Wardman P (1989) Reduction potentials of one-electron couples involving free radicals in aqueous solution. J Phys Chem Ref Data 18: 1637–1755.
  48. 48. Reich JG, Sel’kov EE (1981) Energy metabolism of the cell: a theoretical treatise: Academic Press. 135 p.
  49. 49. Cohen G, Fessl F, Traczyk A, Rytka J, Ruis H (1985) Isolation of the catalase A gene of Saccharomyces cerevisiae by complementation of the cta1 mutation. Mol Gen Genet: 74–79.
  50. 50. Petrova VY, Drescher D, Kujumdzieva AV, Schmitt MJ (2004) Dual targeting of yeast catalase A to peroxisomes and mitochondria. Biochemical J 380: 393–400.
  51. 51. Garcera A, Barreto L, Piedrafita L, Tamarit J, Herrero E (2006) Saccharomyces cerevisiae cells have three Omega class glutathione S-transferases acting as 1-Cys thiol transferases. Biochem J 398: 187–196.
  52. 52. Henke B, Girzalsky W, Berteaux-Lecellier V, Erdmann R (1998) IDP3 encodes a peroxisomal NADP-dependent isocitrate dehydrogenase required for the beta-oxidation of unsaturated fatty acids. J Biol Chem 273: 3702–3711.
  53. 53. Sugiyama K, Kawamura A, Izawa S, Inoue Y (2000) Role of glutathione in heat-shock-induced cell death of Saccharomyces cerevisiae. Biochemical J 352: 71–78.
  54. 54. Kumar C, Igbaria A, D’Autreaux B, Planson AG, Junot C, et al. (2011) Glutathione revisited: a vital function in iron metabolism and ancillary role in thiol-redox control. EMBO J 30: 2044–2056.
  55. 55. Kojer K, Bien M, Gangel H, Morgan B, Dick TP, et al. (2012) Glutathione redox potential in the mitochondrial intermembrane space is linked to the cytosol and impacts the Mia40 redox state. EMBO J 31: 3169–3182.