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Research Article

A Green Fluorescent Protein Containing a QFG Tri-Peptide Chromophore: Optical Properties and X-Ray Crystal Structure

  • Jion M. Battad equal contributor,

    equal contributor Contributed equally to this work with: Jion M. Battad, Daouda A. K. Traore

    Affiliation: Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Daouda A. K. Traore equal contributor,

    equal contributor Contributed equally to this work with: Jion M. Battad, Daouda A. K. Traore

    Affiliation: The Structural Biology Unit, Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Emma Byres,

    Affiliation: The Structural Biology Unit, Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Jamie Rossjohn,

    Affiliation: The Structural Biology Unit, Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Rodney J. Devenish,

    Affiliation: Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Seth Olsen,

    Affiliation: School of Mathematics and Physics, The University of Queensland, Brisbane, Queensland, Australia

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  • Matthew C. J. Wilce mail,

    Mark.Prescott@monash.edu (MP); Matthew.Wilce@monash.edu (MW)

    Affiliation: The Structural Biology Unit, Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Mark Prescott mail

    Mark.Prescott@monash.edu (MP); Matthew.Wilce@monash.edu (MW)

    Affiliation: Department of Biochemistry and Molecular Biology, School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

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  • Published: October 10, 2012
  • DOI: 10.1371/journal.pone.0047331

Abstract

Rtms5 is an deep blue weakly fluorescent GFP-like protein (, 592 nm; , 630nm; ΦF, 0.004) that contains a 66Gln-Tyr-Gly chromophore tripeptide sequence. We investigated the optical properties and structure of two variants, Rtms5Y67F and Rtms5Y67F/H146S in which the tyrosine at position 67 was substituted by a phenylalanine. Compared to the parent proteins the optical spectra for these new variants were significantly blue-shifted. Rtms5Y67F spectra were characterised by two absorbing species (, 440 nm and 513 nm) and green fluorescence emission (, 440 nm; , 508 nm; ΦF, 0.11), whilst Rtms5Y67F/H146S spectra were characterised by a single absorbing species (, 440 nm) and a relatively high fluorescence quantum yield (ΦF, 0.75; , 440 nm; , 508 nm). The fluorescence emissions of each variant were remarkably stable over a wide range of pH (3–11). These are the first GFP-like proteins with green emissions (500–520 nm) that do not have a tyrosine at position 67. The X-ray crystal structure of each protein was determined to 2.2 Å resolution and showed that the benzylidine ring of the chromophore, similar to the 4-hydroxybenzylidine ring of the Rtms5 parent, is non-coplanar and in the trans conformation. The results of chemical quantum calculations together with the structural data suggested that the 513 nm absorbing species in Rtms5Y67F results from an unusual form of the chromophore protonated at the acylimine oxygen. These are the first X-ray crystal structures for fluorescent proteins with a functional chromophore containing a phenylalanine at position 67.

Introduction

GFP-like proteins are valuable tools for use in molecular cell biology applications [1], [2]. Extensive engineering has resulted in a range of proteins whose fluorescence emissions extend over the entire visible range. Many of the proteins have been cloned and developed from a limited number of naturally occurring fluorescent progenitors that include Aequorea victoria GFP (avGFP) [3] and DsRed isolated from Discosoma species [4]. Some non-fluorescent proteins such as hcCP, a chromoprotein isolated from Heteractis crispa have served as a valuable source of far-red fluorescent proteins that include HcRed [5].

Formation of the chromophore in GFP-like proteins is the result of a series of post-translational autocatalytic events involving a tri-peptide motif. All naturally occurring GFP-like proteins isolated to date contain the tri-peptide X-Tyr-Gly, however the tyrosine can be substituted for other amino acids resulting in proteins with different optical properties. For example, substituting the chromophore tyrosine in avGFP with tryptophan or histidine resulted in blue-shifted fluorescent proteins (FPs) with cyan and blue fluorescence emissions, respectively [6]. A phenylalanine substitution results in FPs with the most blue-shifted emissions such as the avGFPY66F (, 442 nm) [7], and the more recently developed Sirius (, 424 nm) [8].

A number of covalent modifications have been identified that further expand the range of optical properties including alternative chromophore structures [9]. For example, the red-shifted optical characteristics of DsRed and eqFP611 are the result of an acylimine linkage extending the chromophore conjugation system [10], [11]. In addition to providing the appropriate environment to promote chromophore formation, contacts between the mature chromophore and the protein matrix determine the optical properties of these proteins. For instance, a Thr203Tyr substitution introduced to avGFP resulted in the first yellow fluorescent protein [12], whilst contacts with the acylimine oxygen are believed to contribute to the red-shifted properties of mPlum and Neptune [13], [14].

Rtms5 is a deep blue weakly fluorescent GFP-like protein (ΦF, 0.004; , 592 nm) isolated from the coral Montipora efflorescens [15]. The X-ray crystal structure of Rtms5 suggests that its low fluorescence emission results from the trans non-coplanar configuration of the chromophore derived from an Gln-Tyr-Gly tripeptide [15]. An Rtms5H146S variant was significantly more fluorescent than Rtms5 particularly at high pH (ΦF, 0.16 at pH 11.0; , 630 nm), and the X-ray crystal structure showed evidence for a chromophore in a cis-coplanar configuration [16]. The chromophore in Rtms5 is extended by the presence of an acylimine linkage, and is in part responsible for the red-shifted optical properties of this protein [15][18].

Remarkably, there are few reports in the literature describing the properties of FPs with a phenylalanine in the chromophore tripeptide (i.e. X-Phe-Gly), and no X-ray crystal structures are available, other than those for proteins that do not have a correctly formed GFP-like chromophore [19]. Therefore, in this study we set out to investigate the optical properties and structure of Rtms5 and Rtms5H146S each containing a Tyr67Phe substitution. The resulting proteins, Rtms5Y67F and Rtms5Y67F/H146S, have green fluorescence emission (, 508 nm), and are the first FPs reported that have both green emissions (500–525 nm) and a phenylalanine in the chromophore tripeptide. The X-ray crystal structure of each of the variants was determined to 2.2 Å resolution. The structures show evidence for the presence of an acylimine linkage extending the chromophore conjugation system that contributed to the green fluorescence emission. The chromophores are in a trans non-coplanar conformation. To our knowledge, these are the first reported X-ray structures for GFP-like proteins containing a functional phenylalanine-substituted chromophore.

Results

Optical Properties of Rtms5Y67F and Rtms5Y67F/H146S

In order to investigate the effects of a tyrosine to phenyalanine substitution in Rtms5 and Rtms5H146S we determined the absorbance and fluorescence spectra for Rtms5Y67F and Rtms5Y67F/H146S at pH 8.0, and compared them to Rtms5 and Rtms5H146S, the parent proteins from which they were derived [15]. The absorbance spectrum for Rtms5Y67F/H146S showed a single species (, 430 nm) whilst the absorbance spectrum for Rtms5Y67F showed two major species (, 440 nm and 513 nm) and a shoulder at ~589 nm (Fig. 1a and b). The fluorescence excitation and emission spectra for Rtms5Y67F and Rtms5Y67F/H146S were similar (, 440 nm; , 508 nm) (Fig. 1), but compared to Rtms5Y67FF, 0.11) the fluorescence quantum yield for Rtms5Y67F/H146SF, 0.75) was somewhat higher. No significant florescence emission was observed when the 513 nm species of Rtms5Y67F was excited. By comparison the tyrosine-containing chromophores of Rtms5 and Rtms5H146S show a single red-shifted absorbing species (Fig 1c and d; , 592 nm and 588 nm, respectively) and very weak fluorescence emissions (ΦF, 0.004 and 0.02 for Rtms5 and Rtms5H146S, respectively). The optical characteristics determined for proteins in this study are summarised and compared to those of other selected proteins in Table 1. Collectively these data indicate that a Tyr to Phe substitution results in Rtms5 variants that have significant blue-shifts in their optical spectra (~150 nm in), and a significant increase in ΦF.

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Figure 1. Absorbance and fluorescence spectra for Rtms5Y67F, Rtms5Y67F/H146S, Rtms5 and Rtms5H146S.

Spectra for Rtms5Y67F, (A); Rtms5Y67F/H146S, (B); Rtms5, (C) and Rtms5H146S, (D) were determined in 20 mM Tris-HCl, pH8.0 and 300 mM NaCl. Absorbance spectra are normalised at 280 nm. Absorbance (solid line), excitation (dashed line), and emission (dotted line).

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Table 1. Optical properties of Rtms5 variants and selected fluorescent proteins.

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Interestingly, compared to the phenylalanine-substituted chromophore of Sirius (, 355 nm), a blue-emitting FP derived from avGFP, the chromophores of Rtms5Y67F and Rtms5Y67F/H146S are red-shifted by ~ 86 nm. Since the Rtms5 and Rtms5H146S chromophores are reported to contain an acylimine linkage (Fig. 2) that extends their conjugation system and contributes to their red-shifted optical properties [15], we were prompted to investigate the possibility that the Rtms5Y67F and Rtms5Y67F/H146S chromophores also contained an acylimine linkage. Acylimine linkages are susceptible to nucleophilic attack, and when present in FPs undergo addition of water across the double bond when the protein is exposed to extremes of pH. Acylimine hydration results in a reduction in the extent of conjugation of the chromophore, and a characteristic blue-shift in its absorbance spectra [10], [17], [20]. Rtms5Y67F or Rtms5Y67F/H146S were incubated in buffer at pH 2.3, and their absorbance spectra determined at selected time points. The acylimine-containing chromophores of Rtms5 and Rtms5H146S were included in this study as positive controls [15]. The results show that incubation of Rtms5Y67F/H146S led to a decrease in the amount of the 400 nm species and a corresponding increase in the amount of a 355 nm species. A single isosbestic point at 375 nm was observed indicating that these two species are stoichiometrically related (Fig. 3b). The blue-shift in the Rtms5Y67F/H146S absorbance spectrum indicates a reduction in the extent of chromophore conjugation resulting from hydration of an acylimine linkage. The control proteins Rtms5 and Rtms5H146S which are known to contain an acylimine linkage [15], [18] undergo a characteristic blue-shift (435 nm to 386 nm) in their absorbance spectra with an isosbestic point at 410 nm (Fig. 3c and d). Collectively, these data indicate that the Rtms5Y67F/H146S chromophore contains an acylimine linkage.

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Figure 2. Chemical structure of the chromophore in Rtms5Y67F and Rtms5Y67F/H146S.

The chemical structure of the mature chromophore is shown. Individual moieties identified in the text are labelled: (1), benzylidine; (2), methine; (3), imidazalinone; (4) glutaminyl; (5), acylimine linkage; and (6) glycyl. The location of the N- and C-termini are indicated.

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Figure 3. The effect of low pH on the absorbance spectra of Rtms5Y67F and Rtms5Y67F/H146S.

Rtms5Y67F (A) and Rtms5Y67F/H146S (B) at a protein concentration of 0.25 mg/ml in 0.1 M potassium phosphate, pH 2.3 were incubated at 21°C and the absorption spectra determined at selected time points. Rtms5 (C) and Rtms5H146S (D) at a protein concentration of 0.30 mg/ml in 0.1 M potassium phosphate, pH 2.3 were included as controls. The first absorbance scan of the incubation mixture (t0) is indicated. Relative trends (decrease or increase) in the absorbance spectra at different positions are indicated by arrows. The kinetics for changes in amount of individual absorbing species for each protein are shown (inset).

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Changes in the absorbance spectrum for Rtms5Y67F incubated at pH 2.3 appeared more complex (Fig. 3a). At low pH a decrease in amounts of the 425 nm and 513 nm species was associated with a corresponding increase in the amount of the 349 nm species. These changes were irreversible as the 425 and 513 nm species did not reappear when the reaction mixture from the end point of the reaction was titrated back to pH 8.0. These results suggest that both the 513 nm and 425 nm chromophore species contain an acylimine linkage. The presence of a single isosbestic point at 390 nm suggests that both the 425 nm and 513 nm species exchange with the 349 nm species. The absence of a clear isosbestic point between the 425 nm and 513 nm species suggests that the 513 nm exchanges with the 390 nm independently of the 425 nm species.

In order to help exclude the possibility that exposure of proteins to low pH contributed to some change in chromophore structure, other than hydrolysis of the acylimine linkage, we investigated the chromophore at pH 8.0 in the presence of a protein denaturant. Guanidine HCl (GuHCl) promotes protein unfolding thereby exposing the chromophore acylimine linkage to the bulk solvent, and subsequent nucleophilic attack and hydration. We incubated Rtms5Y67F and Rtms5Y67F/H146S in 6 M GuHCl at pH 8.0, and determined the absorbance spectra at selected time points. For Rtms5Y67F the amounts of the 515 nm and 453 species decreased, leading to a corresponding increase in the 345 nm species (Fig. 4a). For Rtms5Y67F/H146S the amount of the 435 nm and 340 nm species decreased and increased, respectively (Fig. 4b). Collectively, these results together with those obtained at low pH suggest that all chromophore species in these proteins contain an acylimine linkage, and that the 513 nm species of Rtms5Y67F likely arises from alternate interactions of the chromophore with the protein matrix, and not a separate covalent modification of the Rtms5Y67Fchromophore. Structural evidence presented later supports such a possibility.

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Figure 4. The effect of GuHCl on the absorbance spectra of Rtms5Y67F and Rtms5Y67F/H146S.

Rtms5Y67F (A) and Rtms5Y67F/H146S (B) were diluted to a final protein concentration of 0.15 mg/ml in 0.1 M Tris-HCl (pH 8.0), 6 M GuHCl, and the absorption spectra determined at selected time points after incubation at 21°C. The first absorbance scan (t0) is indicated. Relative trends (decrease or increase) in absorbance are indicated by arrows. The kinetics for individual absorbing species is shown for each protein (inset).

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Finally, we investigated in further detail the effect of pH on the absorbance and fluorescence emission spectra of Rtms5Y67F and Rtms5Y67F/H146S. The absorbance and fluorescence emission for both Rtms5Y67F and Rtms5Y67F/H146S remained remarkably stable over the range pH 3–11 (pKa <3.0 absorbance and emission) (Fig. 5a and b). Changes in absorbance and emission observed outside this pH range (<3 and >11) are likely the result of nucleophilic attack on the acylimine linkage and loss of chromophore conjugation as already discussed (Fig. 3). In comparison absorbance by Rtms5 and Rtms5H146S (, ~ 592 nm) decreases significantly below pH ~ 4 (pKa 3.2 and 4.6 for Rtms5 and Rtms5H146S, respectively) (Fig. 5c and d) [17]. These proteins also show a significant increases in ΦF at pH >10. The 4-hydroxybenzylidine moiety of the Rtms5 and Rtms5H146S chromophores titrates between an anionic form (, ~ 592 nm) and neutral form (, 450nm) [16], whereas the benzylidine moiety of the Rtms5Y67F and Rtms5Y67F/H146S chromophore, lacking a titratable group exists in a neutral form at all pH values (Fig. 2). Collectively these results indicate that the absorbance and fluorescence properties of Rtms5Y67 and in particular Rtms5Y67F/H146S are stable over a wider range of pH compared to their tyrosine-containing counterparts, Rtms5 and Rtms5H146S.

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Figure 5. The effect of pH on the fluorescence emission and absorbance of Rtms5Y67F, Rtms5Y67F/H146S, Rtms5 and Rtms5 H146S.

Absorbance and fluorescence emission spectra were determined at different pH in buffers of constant ionic strength for (A), Rtms5Y67F; (B), Rtms5Y67F/H146S; (C), Rtms5 and (D), Rtms5 H146S. Values shown are those at the and for each protein. Excitation was 440 nm for A and B, and 590 nm for C and D.

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Structural Overview of Rtms5Y67F and Rtms5Y67F/H146S

We have determined the X-ray crystal structure of Rtms5Y67F and Rtms5Y67F/H146S. The crystallography and structural statistics are reported in Table 2. Each of the protomers in Rtms5Y67F and Rtms5Y67F/H146S consist of the same 11-stranded β-can motif (Fig. 6a) typical of members of the GFP-superfamily of proteins. Located at the core of the barrel is the circularised tri-peptide QFG chromophore maintaining covalent links to Cys65 and Ser69 of the main-chain. Within the asymmetric unit of Rtms5Y67F there are 2 tetramers with 222 non-crystallographic symmetry (Fig. 6b) which both match the biological unit predicted by analysis using PISA [21] and the biological unit observed for Rtms5. Rtms5Y67F/H146 is also predicted to form a tetramer with222 non-crystallographic symmetry in the biological unit. The greatest rmsd value between protomer A and its 7 non-crystallographically symmetry related protomers of Rtms5Y67F was 0.134 Å and, as such, the protomers are considered identical. Clear electron density for the Rtms5Y67F chromophore was observed in each protomer with clear links to Cys65 and Ser69 while the density for the Rtms5Y67F/H146S chromophore was more ambiguous.

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Table 2. Rtms5Y67F and Rtms5Y67F/H146S data collection and refinement statistics.

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Figure 6. Rtms5Y67F structure.

A schematic ribbon representation of an isolated protomer (A) of Rtms5Y67F showing the 11-stranded β-can motif typical of GFP-like proteins. The biological assembly as predicted by PISA is a 222 tetramer similar to Rtms5 (B). The chromophore is represented in stick format.

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Chromophore Structure and Environment

In the following section we describe the chromophore structure and environment of Rtms5Y67F and Rtms5Y67F/H146S in relation to the parent protein Rtms5 [15]. Rtms5Y67F and Rtms5Y67F/H146S each contain a benzylidine imidazolinone chromophore derived from the tripeptide Gln-Phe-Gly (Fig. 2). In each variant the Gln66 Cα, originally in the sp3 hybrid conformation is planar and sp2 hybridised as observed for other Rtms5 structures [15], [16], [17]. This arrangement is consistent with the formation of an acylimine linkage extending the π-bonding system of the chromophore as suggested by the red-shifted spectral data (Fig. 3; Fig. 2).

Contacts between the Rtms5Y67F chromophore (glutaminyl, imidazolinone and glycyl moieties) and the protein matrix are similar to those observed for Rtms5 (Table 3; Fig. 7; [15]). However, contacts between the respective protein matrix and the 4-hydroxybenzylidine of Rtms5 or benzylidine of Rtms5Y67F are different. The 4-hydroxybenzylidine of Rtms5 is stabilised by a total of 17 van der Waals (vdw) interactions (Fig. 7b) [15] whereas the benzylidine moiety of Rtms5Y67F is stabilised by only 14 vdw interactions. The vdw interactions in Rtms5Y67F are contributed by His146, Arg197, Asn161, Glu148, Arg97 and Phe177 (Fig. 7a; Table 3).

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Table 3. Rtms5Y67F chromophore contacts.

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Figure 7. The chromophore environment of Rtms5Y67F and Rtms5.

Stereoviews are shown comparing the chromophore environments and H-bonding for Rtms5Y67F (A) and Rtms5 (B). Chromophores are shown in orange (Rtms5Y67F) or blue (Rtms5). H-bonding is indicated by broken lines (corresponding distances are shown in Table 3). Waters are shown as red spheres. Two waters (W1092 and W2932) present in Rtms5Y67F but not Rtms5, that contribute to differences in H-bonding are labelled. The distance between W1092 and Cβ2 of the methine bridge of the Rtms5Y67F chromophore is 2.2 Å and highlighted by a red broken line. H-bonds between the 4-hydroxybenzylidine moiety of Rtms5 and Thr179 (water mediated) and Asn161 are not present in Rtms5Y67F.

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The 4-hydroxybenzylidine moiety of Rtms5 is stabilised by a water-mediated (W310) H-bond with Thr179 and an H-bond with Asn161 (Fig. 7b). However, in the absence of a hydroxyl group the benzylidine moiety of Rtms5Y67F lacks such contacts. As a consequence the side-chain of Asn161 of Rtms5Y67F is rotated around the Cα, and extends towards the 4-hydroxybenzylidine moiety of the Rtms5 chromophore, where Oδ2 maintains a water mediated H-bond with Oγ1 of Thr179, whilst Nδ2 forms an H-bond with Nδ1 of the imidazole ring of His146 (Fig 7a). Since the chromophores in both Rtms5Y67F and Rtms5 are non-coplanar it can be concluded that contact with Thr179 does not contribute to stabilisation of this conformation.

Two waters (W292 and W1092) not observed in Rtms5 or Rtms5Y67F/H146S, contribute to differences in hydrogen bonding around the chromophore of Rtms5Y67F (Fig. 7a). The Nε2 of His146 forms a water-mediated H-bond with Oε1 of Glu215 through water molecule W1092. Notably, this water is within 2.1 Å of Cβ2 of the chromophore methine bridge (Fig. 7a). It is possible that the proximity of W1092 to the methine bridge contributes to the observed red-shift in the absorbance spectrum of Rtms5Y67F compared to that of Rtms5Y67F/H146S (Fig. 1; Table 1) by coordinating increased electron pair density on the bridge of the chromophore [22]. A water-mediated H-bond is maintained between Oε2 of Glu148 and Nε of Arg197 through water A292. Additionally, the Glu215 carboxyl Oε1 H-bonds to N2 of the chromophore imidazolinone ring, while Glu215 Oε2 maintains water-mediated H bonds with Oγ Ser217 and Oγ1 Thr73 through water W292, and a water-mediated H-bond to N2 of the chromophore imidazolinone ring through water W247.

The imidazole ring of His146 in Rtms5Y67F is rotated around Cβ towards the benzylidine ring and contributes to a significant increase in the non-coplanarity of the Rtms5Y67F chromophore compared to the Rtms5 chromophore (Fig. 7a). The benzylidine moiety of Rtms5Y67F is twisted out of plane with respect to the imidazolinone ring with tilt and twist angles of −178° and 53°, respectively averaged across all eight protomers (Table 4) whereas the 4-hydroxybenzylidine ring of Rtms5 is twisted out of plane with respect to the imidazolinone ring with tilt and twist angles of 170° and 43°, respectively [15].

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Table 4. Measured angles for the chromophores of Rtms5 variants and selected fluorescent proteins.

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The different constraints imposed by the protein matrix upon the Rtms5Y67F and Rtms5 chromophores are reflected in the average angle for the Cα2-Cβ2-Cγ2 bond of the methine bridge (Fig. 2). The average angle of 121° for the Cα2-Cβ2-Cγ2 bond in Rtms5Y67F is close to the ideal angle for this bond, compared to angles of 139° and 140° observed in Rtms5 and Rtms5H146S, respectively (Table 4).

Compared to Rtms5Y67F, the structure of the Rtms5Y67F/H146S chromophore is less well defined with B-factors higher than the side-chains of the surrounding residues. A simulated annealing omit map shows that compared to Rtms5Y67F, the Rtms5Y67F/H146S chromophore is not well-defined in the electron density (Fig. 8). This effect may result from a reduced number of chromophore contacts as observed for Rtms5Y67F when compared to Rtms5, together with the additional His146Ser substitution. Nevertheless, sufficient electron density exists to enable the modelling of a trans, non-coplanar Rtms5Y67F/H146S chromophore. As a result of the His146Ser substitution, a pocket exists in Rtms5Y67F/H146S with the potential to accommodate the chromophore in a cis conformation (Fig. S1). In order to investigate the possibility that the Rtms5Y67F/H146S chromophore is mobile and is able to adopt alternate conformations, the trans and cis chromophore conformations were modelled at different occupancies. The difference maps showed increasing amounts of negative density in the position corresponding to the cis conformation as the occupancy of the cis chromophore approaches 1 (Fig. S2). The analysis suggests that the trans conformation of the Rtms5Y67FH146S chromophore is favoured.

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Figure 8. Simulated annealing omit maps for the chromophores of Rtms5Y67F and Rtms5Y67F/H146S.

Alternate views are shown for the non-coplanar chromophores of Rtms5Y67F (A and B; orange) and Rtms5Y67F/H146S (C and D; green). Nearby waters (numbered red spheres) were included in the omit map calculation. The omit map calculation for the Rtms5Y67F/H146S chromophore included a nearby chloride (green sphere). The omit map indicates that the Rtms5Y67F chromophore is in the trans conformation whilst the Rtms5Y67F/H146S chromophore omit map is more ambiguous. The mesh representing the omit maps is contoured to 2.5σ. Difference maps showing the trans and cis Rtms5Y67F/H146S chromophore conformations under different occupancies are shown in Fig. S2.

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Quantum Chemical Calculations

In order to guide the assignment of the absorbance bands of the Rtms5Y67F variants investigated in this study, we performed quantum chemical calculations of the electronic excitation energies of a truncated model of the chromophore. The chemical structure of the chromophore model is shown in Figure 9. The model is truncated at a level consistent with earlier studies of acylimine-substituted FP chromophore models, and includes all atoms that contribute to the π-electron system [23], [24]. We examined four distinct protonation states of the model: an unprotonated neutral form, and three singly protonated forms with the proton bound to the imidazolinone nitrogen site (ImNH+), the imidazolinone oxygen site (ImOH+), and the acylimine oxygen site (AcOH+). The excitation energies and dipole observables associated with the S0–S1 transition of the Rtms5Y67F chromophore model are listed in Table 5.

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Figure 9. The chromophore model used for quantum chemical calculations.

The chromophore model is truncated at a level consistent with earlier studies of acylimine-substituted FP chromophore models. The neutral unprotonated form is shown. The protonation sites for each of the three singly protonated forms are indicated.

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The computational results were obtained for the truncated model in gas phase and any effects of the protein environment, both steric and electronic, are neglected. For this reason, the confidence that one can place on assignments based on these data is determined by the relative separation of the distinct absorbance bands in the proteins and the separation of excitation energies for different states of the model. Fortunately, the excitation energies of most of the states used in the calculations are quite distinguishable. However, we note that in all cases the optimized geometries of the models are planar. Non-planar distortions of the methine bridge are expected to provide a modest red-shift (on the order of 0.1 eV) [24]. Non-planarity of the acylimine linkage is expected to affect the absorbance to a smaller extent, because the conjugation through the imine nitrogen can occur even with significant twisting [23].

Rtms5Y67F but not Rtms5Y67F/H146S has an absorbance band at 513 nm (Fig. 1). The calculated excitation energy of the state protonated at the acylimine oxygen (AcOH+) is significantly redder than the neutral chromophore (368nm) (Table 5). This suggests that the absorbance band near 513 nm, characteristic of Rtms5Y67F should not be attributed to an unprotonated chromophore species. Instead, this band is more reasonably assigned to a species that is protonated at the acylimine oxygen. A difference in the position of the side-chain of Ser69 in Rtms5Y67F compared to Rtms5Y67F/H146S lends support to this idea. The Oγ of Ser 69 and ηOH of Tyr 14 in Rtms5Y67F/H146S are within H-bonding distance of the acylimine oxygen (Fig. 10). Rotation of the Ser69 side-chain and repositioning of the acylimine oxygen in Rtms5Y67F place them beyond hydrogen bonding distance suggesting a change in the charge associated with the acylimine oxygen.

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Table 5. Results of quantum chemistry calculations on neutral and singly protonated forms of the Rtms5Y67F chromophore.

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Figure 10. Chromophore contacts for Rtms5Y67F and Rtms5Y67F/H146S.

Selected contacts are shown for the chromophore of Rtms5Y67F (A) and Rtms5Y67F/H146S (B) highlighting the different positioning of the Ser69 side-chain relative to the acylimine oxygen. The charge associated with acylimine oxygen is thought to explain the existence of the 513 nm absorbing species in Rtms5Y67F.

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Discussion

This is the first report describing an FP with green fluorescence emission (, 500–520 nm) that does not have tyrosine as the aromatic amino acid in the chromophore tripeptide. Only two other FPs, the cyan emitting mBlueberry 2 (, 467 nm) and mBlueberry 1 [25], are presumed to contain the same chromophore structure as Rtms5Y67F and Rtms5Y67F/H146S. mBlueberry 2 was derived from the acylimine-containing red fluorescent mCherry by introduction of number of amino acid substitutions including a Tyr to Phe substitution at position 67. In the absence of a an X-ray crystal structure for mBlueberry 2 the reasons for the marked difference in emission maxima (~ 40 nm) between mBlueberry 2 and the Rtms5Y67F variants (Table 2) are unclear but presumably arise from altered contacts of the chromophore with the surrounding amino acid side-chains. It is known that subtle changes in chromophore contacts can generate significant differences in the emission spectra. For example, the position of the positively charged side-chain of Arg197 relative to the 4-hydroxy benzylidine moiety is, in part, believed to be responsible for producing the significantly red-shifted spectra of mNeptune (, 655 nm) [14]. In Rtms5Y67F the same side-chain of Arg197 is within vdw distance of the benzylidine ring (Table 3; Fig. 7a; Fig. S1) whereas in mBlueberry1 and mBlueberry2 the charged side chain of Arg197 is substituted by the non charged side-chain of isoleucine [25], a change that would be consistent with the blue-shifted spectra observed for the mBlueberry variants.

The weak fluorescence emission observed for both Rtms5 and Rtms5H146SF, 0.004 and 0.02, respectively) has been attributed previously to their trans non-coplanar chromophores [15]. A significant increase in fluorescence emission (20-fold; ΦF, 0.16) observed for Rtms5H146S at alkaline pH (see Fig. 5d) was accompanied by an increased proportion of a cis-coplanar chromophore as observed in the X-ray crystal structure [16]. Since Rtms5Y67F and Rtms5Y67F/H146S are considerably more fluorescent (ΦF, 0.11 and 0.75, respectively) compared to their Rtms5 parents, we were surprised by the lack of evidence for a cis-coplanar chromophore in their structures. The poor electron density corresponding to the chromophore in Rtms5Y67F/H146S suggests it is mobile, and may adopt alternate conformations. However, the difference maps for trans and cis Rtms5Y67F/H146S chromophore conformations under different occupancies indicated that the trans conformation is favoured (Fig. S2) leaving no clear explanation for the increased ΦF of these proteins.

The chromophores in each of the bright red fluorescent EqFP611 and TagRFP [26], [27] are trans-coplanar suggesting that in different proteins a cis or trans chromophore can be highly fluorescent, providing they can adopt a coplanar conformation. It is possible that the fluorescent chromophore species in Rtms5Y67F/H146S is trans-coplanar. Our data for Rtms5Y67F/H146S show that contact between the benzylidine moiety of the chromophore and the side-chain of Arg197 prevents a coplanar conformation (Fig. S1). We attempted to model an alternative orientation of the Arg197 side-chain that allows a coplanar chromophore (Fig. S3). In this model the distance between the side-chain of Arg197 and the benzylidine ring has increased providing the room to accommodate a coplanar chromophore (Fig. S3c and d). In the case of the non-coplanar chromophore stabilisation of the Arg197 side-chain is provided by contact with the side chain of Glu148 and H-bonds mediated by W329 and W319 (Fig. S3a and b), whereas in the case of the coplanar chromophore, stabilisation is provided by H-bonds mediated through W329, W319 and W282 (Fig. S3c and d). How and when movement of the Arg197 side-chain takes place in Rtms5Y67F/H146S is not clear. However, repositioning of the side-chain of a histidine at the same amino acid location is a key feature of the molecular mechanism for photoswitching of DronPA [28]. On illumination with excitation light repositioning of His197 in DronPA promotes isomerisation of the chromophore from a trans non-coplanar, non fluorescent form to a cis coplanar, brightly fluorescent form. If our model is correct Rtms5Y67F/H146S and Rtms5 belong to very small group of FPs that have a fluorescent trans chromophore conformation. Further studies of Rtms5Y67F/H146S are required to investigate the validity of this model.

We were intrigued as to the source of the 513 nm species in Rtms5Y67F. The results of chemical quantum calculations suggest this species may arise from a protonation event involving the acylimine oxygen (AcOH+; Scheme 2). This idea is given additional support by the structural data that suggests a change in the position of the side-chain of Ser 69 in Rtms5Y67F compared to Rtms5Y67F/H146S (Fig. 9). Interaction of the acylimine oxygen with the protein matrix appears to be important for generating a red-shift in the spectra of other FPs [29]. A hydrogen bond between the side-chain of Glu16 and the acylimine carbonyl has been suggested to be important for generating the red-shifted optical spectra of the far-red fluorescent mPlum [13].

The data in Table 5 also suggest that the absorbance band near 440 nm (Fig. 1), characteristic of both Rtms5Y67F and Rtms5Y67F/H146S should not be attributed to an unprotonated chromophore species. Instead, this band is more reasonably assigned to a species that is protonated at either the nitrogen (ImNH+) or oxygen site (ImOH+) on the imidazolinone ring. Although the excitation energy calculated for the ImOH+ model is closer to the experimentally measured energy gap, the weight of precedent favors assignment to a nitrogen-protonated ImNH+ species. Protonation at either of these two positions might be expected be reflected in altered chromophore/protein matrix contacts. Although differences exist in the H-bond network around the chromophore in the RtmsY67F variants compared to their tyrosyl-containing counterparts (Rtms5 and Rtms5H146S) (Fig. 7) in each case an H-bond exists between N2 and O2 of the imidazalinone ring and the Glu215 carboxyl and Arg95, respectively (Fig. 7). We have previously reported that the Rtms5 chromophore is not protonated [16], [30].

There are few reports in the literature of FPs containing a phenylalanine in position 67 of the chromophore. The phenylalanine substituted variants reported here represent an alternative platform on which to develop fluorescent proteins with green emissions (500–520 nm) and superior pH stability. These proteins may also have a fluorescent trans chromophore conformation. Rtms5Y67F and Rtms5Y67F/H146S have the most pH-stable (pKa, 3.5) green emissions of any FPs (500–520 nm) reported to date. The green emissions of Sapphire FPs having been reported previously to be the most stable to pH (pKa 4.9) [31]. This feature of Rtms5Y67F and Rtms5Y67F H146S can be attributed to the benzylidine moiety which lacks a titratable group. The chromophore of the pH-stable blue-emitting Sirius contains the same benzylidine moiety, and has a pKa <3.0 [8]. The Sapphire chromophore contains a 4-hydroxy benzylidine moiety [31]. The ability of Rtms5Y67F and Rtms5Y67F/H146S to fluoresce with little attenuation down to ~ pH 3.5, may prove useful for engineering new improved biosensors for monitoring autophagy in live cells [32]. Autophagy is an important cellular process characterised by the delivery of material to the acidic (pH 4.8) lumen of the lysosome for degradation.

Rtms5Y67F and Rtms5Y67F/H146S are obligate tetramers. However, we recently described a monomer of Rtms5 called Ultramarine [33] that represents a starting point to develop monomer forms of the phenylalanine-substituted FPs, thereby allowing them to be used as fusion partners with other proteins of interest.

Materials and Methods

Mutagenesis, Protein Expression and Purification

Expression vectors encoding Rtms5Y67F or Rtms5Y67F/H146S were constructed by site-directed mutagenesis (QuickChange, Invitrogen) using the primer pair 5′-caccacagtgtcagttcggaagcataccattc-3′ and 5′-gaatggtatgcttccgaactgacactgtggtg-3′ and expression vectors pQE10:Rtms5 or pQE10:Rtms5H146S as templates.

Rtms5Y67F and Rtms5Y67F/H146S proteins were expressed in the NovaBlue (λDE3) strain of E. coli (Novagen) and purified by Ni-NTA chromatography as described [15]. For crystallization purposes proteins were subjected to chromatography on a S200 size exclusion column equilibrated in 20 mM Tris-HCl, pH 8.0, 300 mM NaCl. Fractions containing Rtms5Y67F or Rtms5Y67F/H146S tetramer were pooled and concentrated to 15 mg.ml−1 ready for crystallization trials by the hanging drop vapour diffusion technique.

Spectrometry

Fluorescence spectra were determined using a Varian Eclipse fluorescence spectrophotometer (Melbourne, Australia). ΦF values were determined for proteins (in 20 mM Tris–HCl (pH 8.0), 300 mM NaCl) at 25°C as described [15], [34] using solutions of Rhodamine 101 (ΦF, 1.0) in buffer as standard. Absorbance spectra were determined using a Varian Cary 50 spectrophotometer. For pH titrations, proteins in 20 mM Tris-HCl (pH 8.0) were diluted (~100-fold) as required into selected 0.1 M buffers [16], [17]. Absorbance spectra were recorded at 24°C after 30 sec gentle mixing. Sample pH was monitored using a micro-pH probe. Data from a single a determination are presented.

Crystallization and Structural Determination

Crystals of Rtms5Y67F and Rtms5Y67F/H146S that appeared brown or pale green, respectively were obtained at 20°C via the hanging drop method. Protein (15 mg.ml−1) in 20 mM Tris, 300 mM NaCl, pH 8.0 was mixed 1:1 or 1:2 with crystallization solutions, respectively. Numerous small crystals were obtained using conditions reported for Rtms5 [15], [16], [17]. Further optimisation of the crystallisation conditions led to diffraction quality crystals. Rtms5Y67F crystals (0.1–0.2 mm in length) were obtained using a crystallization solution composed of 22% PEG 3350 and 0.34 M KI buffered with 0.2 M Tris-HCl pH 8.5 in 3 µl hanging drops (1:2 protein/crystallization solution ratio). Rtms5Y67H/H146S crystals 0.1–0.2 mm in length were obtained using a crystallization solution with 21% PEG 3350, 0.36 M KI, and 25% glycerol buffered with 0.2 M Tris pH 8.5 in 3 µl hanging drops (1:2 protein/crystallization solution ratio). Rtms5Y67F crystals were flash frozen prior to data collection using 30% (v/v) glycerol in the precipitant as cryoprotectant. Crystals were transferred stepwise (5% increments) into increasing amounts of glycerol over a time period of 2 h. Rtms5Y67F/H146S crystals were dipped in perfluoropolyether oil (PFO-X175/08, Hampton Research) for 1 min before vitrification in a nitrogen-gas stream maintained at 100 K.

Diffraction images for Rtms5Y67F and Rtms5Y67H/H146S were collected at the APS IMCA-CAT beamline in Chicago (USA), and at the MX-1 beamline of the Australian Synchrotron, respectively.

Data integration was carried out with the HKL software package (http://www.hkl-xray.com) [35] for Rtms5Y67F and with XDS (http://xds.mpimf-heidelberg.mpg.de) [36] for Rtms5Y67F/H146S. Molecular replacement for both Rtms5Y67F and Rtms5Y67F/H146S was carried out with Phaser [37] included in the CCP4 program suite (http://www.ccp4.ac.uk/ccp4i_main.php) [38]. The initial search probe used in Phaser was the wild-type Rtms5 model (1MOV) trimmed of water molecules, residue 146, and the chromophore. The top-scoring Phaser solution for Rtms5Y67F consists of 8 protomers arranged into a pair of 222 tetramers in its asymmetric unit while the top-scoring solution for Rtms5Y67F/H146S had a single protomer in the asymmetric unit.

Restrained refinement of Rtms5Y67F and Rtms5Y67F/H146S models was carried out in Refmac5 [39] with automatic weighting interspersed with rounds of model building in WinCoot (http://www.ysbl.york.ac.uk/~lohkamp/coot​/wincoot.html) [40]. TLS refinement was used in the last few rounds of refinement in Refmac5. Models were checked with Molprobity (http://molprobity.biochem.duke.edu) [41] to guide model building. Tight main-chain and medium side-chain NCS restraints were applied in Refmac5 to residues 8–223 in early rounds of refinement of Rtms5Y67F which was relaxed in later rounds of refinement. Rounds of simulated annealing refinement in Phenix (http://www.phenix-online.org) [42] were used to reduce bias and calculate difference omit maps to guide model building. Water molecules were placed into peaks in the FO-FC map and kept in the model if they were located within hydrogen-bonding distance of chemically reasonable groups, visible at 3.0σ map contour level, and possessed a B-factor <80 Å2. Strong peaks observed in the FO-FC map too large to be waters were modelled as chloride ions while even stronger peaks were modelled as iodide ions (both included in the crystallization conditions).

The monomer library definitions and PDB coordinates of the QFG chromophore were created using the CCP4 Monomer Library Sketcher [43] by inputting then editing the coordinates of the wild-type CRQ chromophore. The QFG chromophores were then placed into the electron density using WinCoot. A chloride ion was placed into density near the Rtms5Y67F/H146S chromophore proximal to Ser146 in a position shown to be accessible to halides in Rtms5H146S [17].

Validation of the final Rtms5Y67F and Rtms5Y67F/H146S models prior to deposition through PDBj ADIT was carried out using Molprobity along with SFcheck [44], Procheck [45], and Rampage [46] from the CCP4 software suite. The final Rtms5Y67F model was refined to Rfactor 15.42% and Rfree 19.77% with 98.6% and 1.4% of residues in the favored and allowed regions of the Ramachandran plot, respectively, with none in the generously or disallowed regions. The final Rtms5Y67F/H146S model was refined to Rfactor 19.68% and Rfree 23.99% with 98.1% and 1.4% of residues in the favored and allowed regions of the Ramachandran plot, respectively, with none in the generously or disallowed regions. The coordinates and structure factors for Rtms5Y67F and Rtms5Y67F/H146S have been deposited in the Protein Data Bank (3VIC and 3VK1, respectively). Biological assemblies for Rtms5Y67F and Rtms5Y67F/H146S were predicted using PISA included in the CCP4 program suite [21]. A summary of data collection and refinement statistics is presented in Table 2.

Quantum Chemical Calculations

For each protonation state examined, we optimized the geometry of the model using Møller-Plessett 2nd order perturbation theory [47] and a cc-pvdz basis set [48] (MP2//cc-pvdz). At these geometries, we calculated the excitation energies, transition dipole and difference dipole moments using multi-state multi-reference 2nd order perturbation theory [49], [50] on a four-electron, three-orbital two-state averaged complete active space self-consistent field wavefunction, again with a cc-pvdz basis set [48] (SA2-CAS(4,3)*MS-MRPT2//cc-pvdz). This protocol has previously been used to study the halochromism of GFP chromophore models [51], [52], [53]. All calculations were carried out using the MOLPRO software package (http://www.molpro.net) [54].

Supporting Information

Figure S1.

The chromophore cavities of Rtms5Y67F and Rtms5Y67F/H146S. Orthogonal cutaway views are shown for Rtms5Y67F (A and B) and Rtms5Y67F/H146S (C and D). The side-chain of His146 stabilises the trans conformation of the Rtms5Y67F chromophore. The His146Ser substitution (C) creates a pocket with the potential to accommodate an Rtms5Y67F/H146S chromophore with a cis conformation. The non-coplanar conformation of the chromophores in both Rtms5Y67F and Rtms5Y67F/H146S is stabilised by the side-chains of Arg96 and Arg197 (C and D). Waters are shown as red spheres.

doi:10.1371/journal.pone.0047331.s001

(TIF)

Figure S2.

Difference maps showing the trans and cis Rtms5Y67F/H146S chromophore conformations under different occupancies. Occupancy ratios (trans/cis) are 0.0/1.0, (A); 0.25/0.75, (B); 0.5/0.5, (C); 0.75/0.25, (D) and 1.0/0.0 (E). The positive (green mesh) and negative (red mesh) difference maps are contoured to +2.5σ and −2.5σ, respectively. The trans chromophore conformation is favoured in Rtms5Y67F/H146S. A nearby chloride ion (green sphere) was omitted from the map calculation.

doi:10.1371/journal.pone.0047331.s002

(TIF)

Figure S3.

A model showing the chromophore cavity of Rtms5Y67F/H146S with a hypothetical trans-coplanar chromophore. Orthogonal views of the trans Rtms5Y67F/H146S chromophore in a trans non-coplanar as suggested by the X-ray structure (A and B), and modelled in a trans coplanar conformation (C and D) are shown. The conformation of the Arg197 residue, which contacts the benzylidene moiety of the chromophore (pink dashed lines, distances in Å numbered in pink) restricts the possibility of a trans coplanar chromophore (A). The conformation of Arg197 is stabilised by H-bonds (black dashed lines, distances in Å shown numbered in black) to two nearby water molecules (red spheres, numbered in red) and to Glu148 (B). Repositioning of the Arg197 side chain (C) creates a space in which a trans coplanar chromophore could be accomodated. The side-chain of Arg197 in is stabilised by different contacts (D). A nearby chloride is shown (green sphere). The hypothetical model was created in WinCoot, avoiding major clashes with nearby atoms, and only the rearrangment of the Arg197 side chain has been considered.

doi:10.1371/journal.pone.0047331.s003

(TIF)

Figure S4.

Hypothetical resonance structures for the chromophore model.

doi:10.1371/journal.pone.0047331.s004

(TIF)

Text S1.

doi:10.1371/journal.pone.0047331.s005

(DOCX)

Scheme S1.

doi:10.1371/journal.pone.0047331.s006

(TIF)

Scheme S2.

doi:10.1371/journal.pone.0047331.s007

(TIF)

Author Contributions

Conceived and designed the experiments: JB MP SO DT. Performed the experiments: JB DT EB SO. Analyzed the data: JB DT MP EB JR MW SO. Contributed reagents/materials/analysis tools: MP JR MW. Wrote the paper: JB DT RD MW MP.

References

  1. 1. Shaner NC, Patterson GH, Davidson MW (2007) Advances in fluorescent protein technology. J Cell Sci 120: 4247–4260. doi: 10.1242/jcs.005801
  2. 2. Chudakov DM, Matz MV, Lukyanov S, Lukyanov KA (2010) Fluorescent proteins and their applications in imaging living cells and tissues. Physiol Rev 90: 1103–1163. doi: 10.1152/physrev.00038.2009
  3. 3. Chalfie M, Tu Y, Euskirchen G, Ward WW, Prasher DC (1994) Green fluorescent protein as a marker for gene expression. Science 263: 802–805. doi: 10.1126/science.8303295
  4. 4. Matz MV, Fradkov AF, Labas YA, Savitsky AP, Zaraisky AG, et al. (1999) Fluorescent proteins from nonbioluminescent Anthozoa species. Nat Biotechnol 17: 969–973. doi: 10.1038/13657
  5. 5. Gurskaya NG, Fradkov AF, Terskikh A, Matz MV, Labas YA, et al. (2001) GFP-like chromoproteins as a source of far-red fluorescent proteins. FEBS Lett. 507: 16–20. doi: 10.1016/s0014-5793(01)02930-1
  6. 6. Heim R, Prasher DC, Tsien RY (1994) Wavelength mutations and posttranslational autoxidation of green fluorescent protein. Proc Natl Acad Sci U S A. 91: 12501–12504. doi: 10.1073/pnas.91.26.12501
  7. 7. Cubitt AB, Heim R, Adams SR, Boyd AE, Gross LA, et al. (1995) Understanding, improving and using green fluorescent protein. Trends Biochem Sci. 20: 448–455. doi: 10.1016/s0968-0004(00)89099-4
  8. 8. Tomosugi W, Matsuda T, Tani T, Nemoto T, Kotera I, et al. (2009) An ultramarine fluorescent protein with increased photostability and pH insensitivity. Nat Methods 6: 351–353. doi: 10.1038/nmeth.1317
  9. 9. Wachter RM, Watkins JL, Kim H (2010) Mechanistic diversity of red fluorescence acquisition by GFP-like proteins. Biochemistry 49: 7417–7427. doi: 10.1021/bi100901h
  10. 10. Gross LA, Baird GS, Hoffman RC, Baldridge KK, Tsien RY (2000) The structure of the chromophore within DsRed, a red fluorescent protein from coral. Proc Natl Acad Sci U S A 97: 11990–11995. doi: 10.1073/pnas.97.22.11990
  11. 11. Wiedenmann J, Schenk A, Röcker C, Girod A, Spindler KD, et al. (2002) A far-red fluorescent protein with fast maturation and reduced oligomerization tendency from Entacmaea quadricolor (Anthozoa, Actinaria). Proc Natl Acad Sci U S A. 99: 11646–11651. doi: 10.1073/pnas.182157199
  12. 12. Cubitt AB, Woollenweber LA, Heim R (1999) Understanding structure-function relationships in the Aequorea victoria green fluorescent protein. Methods Cell Biol 58: 19–30. doi: 10.1016/s0091-679x(08)61946-9
  13. 13. Shu X, Wang L, Colip L, Kallio K, Remington SJ (2008) Unique interactions between the chromophore and glutamate 16 lead to far-red emission in a red fluorescent protein. Protein Sci. 18: 460–466. doi: 10.1002/pro.66
  14. 14. Lin MZ, McKeown MR, Ng H, Aguilera TA, Shaner NC, et al. (2009) Autofluorescent Proteins with Excitation in the Optical Window for Intravital Imaging in Mammals. J. Chembiol. 16: 1169–1179. doi: 10.1016/j.chembiol.2009.10.009
  15. 15. Prescott M, Ling M, Beddoe T, Oakley AJ, Dove S, et al. (2003) The 2.2 A crystal structure of a pocilloporin pigment reveals a nonplanar chromophore conformation. Structure. 11: 275–284. doi: 10.1016/s0969-2126(03)00028-5
  16. 16. Battad JM, Wilmann PG, Olsen SC, Byres E, Smith SC, et al. (2007) A Structural Basis for the pH-dependent Increase in Fluorescence Efficiency of Chromoproteins. J Mol Biol 368: 998–1010. doi: 10.1016/j.jmb.2007.02.007
  17. 17. Wilmann PG, Battad JM, Beddoe T, Olsen S, Smith SC, et al. (2006) The 2.0 angstroms crystal structure of a pocilloporin at pH 3.5: the structural basis for the linkage between color transition and halide binding. Photochem Photobiol 82: 359–366. doi: 10.1562/2005-05-02-ra-509
  18. 18. Turcic K, Pettikiriarachchi A, Battad J, Wilmann PG, Rossjohn J, et al. (2006) Amino acid substitutions around the chromophore of the chromoprotein Rtms5 influence polypeptide cleavage. Biochem Biophys Res Commun 340: 1139–1143. doi: 10.1016/j.bbrc.2005.12.118
  19. 19. Barondeau DP, Kassmann CJ, Tainer JA, Getzoff ED (2007) The case of the missing ring: radical cleavage of a carbon-carbon bond and implications for GFP chromophore biosynthesis. J Am Chem Soc. 129: 3118–3126. doi: 10.1021/ja063983u
  20. 20. Pakhomov AA, Pletneva NV, Balashova TA, Martynov VI (2006) Structure and reactivity of the chromophore of a GFP-like chromoprotein from Condylactis gigantea. Biochemistry. 45: 7256–7264. doi: 10.1021/bi060207q
  21. 21. Olsen S (2012) A quantitative quantum chemical model of the Dewar–Knott color rule for cationic diarylmethanes. Chem. Phys. Lett. 532: 106–109. doi: 10.1016/j.cplett.2012.02.047
  22. 22. Krissinel E, Henrick K (2007) Inference of macromolecular assemblies from crystalline state. J Mol Biol. 372: 774–797. doi: 10.1016/j.jmb.2007.05.022
  23. 23. Olsen SC, Smith SC (2006) Trans–cis Isomerism and acylimine formation in DsRed chromophore models: Intrinsic rotation barriers. Chem. Phys. Lett. 426: 159–162. doi: 10.1016/j.cplett.2006.05.020
  24. 24. Olsen SC, Smith SC (2007) Radiationless decay of red fluorescent protein chromophore models via twisted intramolecular charge-transfer states. J. Am. Chem. Soc. 129: 2054–2065. doi: 10.1021/ja066430s
  25. 25. Ai HW, Shaner NC, Cheng Z, Tsien RY, Campbell RE (2007) Exploration of new chromophore structures leads to the identification of improved blue fluorescent proteins. Biochemistry 46: 5904–5910. doi: 10.1021/bi700199g
  26. 26. Petersen J, Wilmann PG, Beddoe T, Oakley AJ, Devenish RJ, et al. (2003) The 2.0-Å Crystal Structure of eqFP611, a Far Red Fluorescent Protein from the Sea Anemone Entacmaea quadricolor. J. Biol. Chem. 278: 44626–44631. doi: 10.1074/jbc.m307896200
  27. 27. Subach OM, Malashkevich VN, Zencheck WD, Morozova KS, Piatkevich KD, et al (2010) Structural characterization of acylimine-containing blue and red chromophores in mTagBFP and TagRFP fluorescent proteins. Chem Biol. 17: 333–341. doi: 10.1016/j.chembiol.2010.03.005
  28. 28. Andresen M, Stiel AC, Trowitzsch S, Weber G, Eggeling C, et al. (2007) Structural basis for reversible photoswitching in Dronpa. Proc Natl Acad Sci U S A. 104: 13005–13009. doi: 10.1073/pnas.0700629104
  29. 29. Chica RA, Moore MM, Allen BD, Mayo SL (2010) Generation of longer emission wavelength red fluorescent proteins using computationally designed libraries. Proc Natl Acad Sci U S A. 107: 20257–20262. doi: 10.1073/pnas.1013910107
  30. 30. Olsen S, Prescott M, Wilmann P, Battad J, Rossjohn J, et al. (2006) Determination of chromophore charge states in the low pH colour transition of the fluorescent protein Rtms5H146S via time-dependent DFT. Chemical Physical Letters. 420: 507–511. doi: 10.1016/j.cplett.2006.01.021
  31. 31. Zapata-Hommer O, Griesbeck O (2003) Efficently folding and circularly permuted variants of the Sapphire mutant of GFP. BMC Biotechnol. 3: 5.
  32. 32. Rosado CJ, Mijaljica D, Hatzinisiriou I, Prescott M, Devenish RJ (2008) Rosella: a fluorescent pH-biosensor for reporting vacuolar turnover of cytosol and organelles in yeast. Autophagy. 4: 205–213.
  33. 33. Pettikiriarachchi A, Gong L, Perugini MA, Devenish RJ, Prescott M (2012) Ultramarine, a chromoprotein acceptor for förster resonance energy transfer. PLoS One. 7: e41028. doi: 10.1371/journal.pone.0041028
  34. 34. Lackowicz JR (1983) Principles of Fluorescence Spectrometry. New York: Plenum Press. 954 p.
  35. 35. Otwinowski Z, Minor W (1997) Processing of X-ray Diffraction Data Collected in Oscillation Mode. In: Carter CW Jr, Sweet RM, editors. Methods in Enzymology 276: Macromolecular Crystallography, part A. New York: Academic Press. 307–326.
  36. 36. Kabsch W (2010) XDS. Acta Crystallogr D Biol Crystallogr. 66: 125–132. doi: 10.1107/s0907444909047337
  37. 37. McCoy AJ, Grosse-Kunstleve RW, Adams PD, Winn MD, Storoni LC, et al. (2007) Phaser crystallographic software. J Appl Crystallogr. 40: 658–674. doi: 10.1107/s0021889807021206
  38. 38. Winn MD, Ballard CC, Cowtan KD, Dodson EJ, Emsley P, et al. (2011) Overview of the CCP4 suite and current developments. Acta Crystallogr D Biol Crystallogr. 67: 235–242. doi: 10.1107/s0907444910045749
  39. 39. Winn MD, Murshudov GN, Papiz MZ (2003) Macromolecular TLS refinement in REFMAC at moderate resolutions. Methods Enzymol. 374: 300–321. doi: 10.1016/s0076-6879(03)74014-2
  40. 40. Emsley P, Lohkamp B, Scott WG, Cowtan K (2010) Features and development of Coot. Acta Crystallogr D Biol Crystallogr. 66: 486–501. doi: 10.1107/s0907444910007493
  41. 41. Chen VB, Arendall WB 3rd, Headd JJ, Keedy DA, Immormino RM, et al (2010) MolProbity: all-atom structure validation for macromolecular crystallography. Acta Crystallogr D Biol Crystallogr. 66: 12–21. doi: 10.1107/s0907444909042073
  42. 42. Adams PD, Afonine PV, Bunkóczi G, Chen VB, Davis IW, et al. (2010) PHENIX: a comprehensive Python-based system for macromolecular structure solution. Acta Crystallogr D Biol Crystallogr. 66: 213–221. doi: 10.1107/s0907444909052925
  43. 43. Vagin AA, Steiner RA, Lebedev AA, Potterton L, McNicholas S, et al. (2004) REFMAC5 dictionary: organization of prior chemical knowledge and guidelines for its use. Acta Crystallogr D Biol Crystallogr. 60: 2184–2195. doi: 10.1107/s0907444904023510
  44. 44. Vaguine AA, Richelle J, Wodak SJ (1999) SFCHECK: a unified set of procedures for evaluating the quality of macromolecular structure-factor data and their agreement with the atomic model. Acta Crystallogr D Biol Crystallogr. 55: 191–205. doi: 10.1107/s0907444998006684
  45. 45. Laskowski RA, MacArthur MW, Moss DS, Thornton JM (1993) PROCHECK - a program to check the stereochemical quality of protein structures. J. App. Cryst. 26: 283–291. doi: 10.1107/s0021889892009944
  46. 46. Lovell SC, Davis IW, Arendall WB 3rd, de Bakker PI, Word JM, et al (2003) Structure validation by Calpha geometry: phi,psi and Cbeta deviation. Proteins. 50: 437–450.
  47. 47. Azhary AE, Rauhut G, Pulay P, Werner H-J (1998) Analytical energy gradients for local second-order Møller-Plesset perturbation theory. J. Chem. Phys. 108: 5185–5193. doi: 10.1063/1.475955
  48. 48. Dunning TH (1989) Gaussian basis sets for use in correlated molecular calculations. I. The atoms boron through neon and hydrogen. J. Chem. Phys. 90: 1007–1023. doi: 10.1063/1.456153
  49. 49. Finley J, Malmqvist P-A, Roos BJ, Serrano-Andrés L (1998) The multi-state CASPT2 method. Chem. Phys. Lett. 288: 299–306. doi: 10.1016/s0009-2614(98)00252-8
  50. 50. Celani P, Werner H (2000) Multireference perturbation theory for large restricted and selected active space reference wave functions. J. Chem. Phys. 112: 5546–5557. doi: 10.1063/1.481132
  51. 51. Olsen S (2010) A Modified Resonance-Theoretic Framework for Structure−Property Relationships in a Halochromic Oxonol Dye. J. Chem. Theory Comput. 6: 1089–1103. doi: 10.1021/ct100001b
  52. 52. Olsen S, Mckenzie RH (2010) A dark excited state of fluorescent protein chromophores, considered as Brooker dyes. Chem. Phys. Lett. 492: 150–156. doi: 10.1016/j.cplett.2010.04.024
  53. 53. Olsen S, Mckenzie RH (2011) Bond alternation, polarizability, and resonance detuning in methine dyes. J. Chem. Phys. 134: 114520–114513. doi: 10.1063/1.3563801
  54. 54. Werner H-J, Knowles PJ, Knizia G, Manby FR, Schütz M (2012) Molpro: a general-purpose quantum chemistry program package. WIREs Comput Mol Sci. 2: 242–253. doi: 10.1002/wcms.82