Erv1 (essential for respiration and viability 1), is an essential component of the MIA (mitochondrial import and assembly) pathway, playing an important role in the oxidative folding of mitochondrial intermembrane space proteins. In the MIA pathway, Mia40, a thiol oxidoreductase with a CPC motif at its active site, oxidizes newly imported substrate proteins. Erv1 a FAD-dependent thiol oxidase, in turn reoxidizes Mia40 via its N-terminal Cys30–Cys33 shuttle disulfide. However, it is unclear how the two shuttle cysteine residues of Erv1 relay electrons from the Mia40 CPC motif to the Erv1 active-site Cys130–Cys133 disulfide. In the present study, using yeast genetic approaches we showed that both shuttle cysteine residues of Erv1 are required for cell growth. In organelle and in vitro studies confirmed that both shuttle cysteine residues were indeed required for import of MIA pathway substrates and Erv1 enzyme function to oxidize Mia40. Furthermore, our results revealed that the two shuttle cysteine residues of Erv1 are functionally distinct. Although Cys33 is essential for forming the intermediate disulfide Cys33–Cys130′ and transferring electrons to the redox active-site directly, Cys30 plays two important roles: (i) dominantly interacts and receives electrons from the Mia40 CPC motif; and (ii) resolves the Erv1 Cys33–Cys130 intermediate disulfide. Taken together, we conclude that both shuttle cysteine residues are required for Erv1 function, and play complementary, but distinct, roles to ensure rapid turnover of active Erv1.
Disulfide bond formation is important for folding and function of many proteins, and it plays an essential role during the biogenesis of mitochondrial IMS (intermembrane space) proteins [1–4]. In Saccharomyces cerevisiae, all the mitochondrial IMS proteins are encoded by the nuclear genome. After protein translation in the cytosol, many of the IMS precursor proteins are imported into mitochondria through the IMS MIA (mitochondrial import and assembly) pathway, which consists of two essential components, Mia40 and a FAD-dependent thiol oxidase Erv1 (essential for respiration and viability 1) [1–3]. Most substrates of the MIA system are small cysteine-rich proteins with conserved twin CX3C [e.g. Tim9 (translocase of the inner membrane) and Tim10] or twin CX9C [e.g. Cox17 (cytochrome c oxidase 17) and hMia40 (human Mia40)] motifs. These substrates are imported into the mitochondrial IMS in a cysteine-reduced unfolded conformation [5–7]. Upon import into the mitochondria, they interact with oxidized Mia40 and form an intermolecular disulfide-bonded substrate–Mia40 complex, leading to disulfide transfer from Mia40 to the substrate and thus trapping the oxidized substrate in the IMS.
All Mia40 proteins contain three pairs of disulfide bonds in a highly conserved C-terminal domain. Although the two disulfides formed between the twin CX9C motifs are stable and play a structural role, a redox-active disulfide bond is formed between cysteine residues in the CPC motif, e.g. Cys296–Cys298 in yeast Mia40 [8–10]. The structures of yeast and hMia40 revealed the presence of a hydrophobic binding cleft in close proximity to the CPC motif redox active site, which plays an important role in driving protein–protein interaction and the recognition of specific substrates [9,10]. Structural data suggest that the second cysteine residue of the CPC motif is more exposed than the first cysteine on the hydrophobic binding cleft, and is therefore better positioned for covalent interaction with its substrate proteins. Consistently, several mixed disulfide intermediates have been identified, forming between the second cysteine of the CPC motif and a docking cysteine of substrate proteins (e.g. the small Tim proteins and Cox17) [10,11]. Upon disulfide transfer to substrate protein, the Mia40 CPC motif is reduced. Subsequently, the reduced Mia40 is reoxidized by Erv1 to restore its function. Thus Mia40 is a substrate (electron donor) of Erv1; Erv1 assists and catalyses the Mia40-dependent import and oxidative protein folding in the mitochondrial IMS. It is worth mentioning that, although a fraction of the Mia40 CPC motif binds iron or an iron–sulfur cluster in vivo, this cofactor-containing Mia40 seems not to act as electron donor for Erv1 .
Erv1 belongs to the single domain ERV/ALR thiol oxidase subfamily, including the mammalian homologue ALR (augmenter of liver regeneration), plant Erv1 [AtErv1 (Arabidopsis thaliana Erv1)], yeast Erv2 [ScErv2 (S. cerevisiae Erv2)] of the ER (endoplasmic reticulum) lumen and other Erv proteins (Figure 1). ERV/ALR enzymes are characterized by a highly conserved FAD-binding catalytic core domain of approximately 100 amino acids containing a CXXC redox active-site disulfide (Cys130–Cys133 in Erv1) located proximally to the isoalloxazing ring of the FAD cofactor (also known as proximal disulfide) and a C-terminal CX16C structural disulfide (Cys159–Cys176 in Erv1). In addition, there is a third disulfide bond (Cys30–Cys33 in Erv1) located either on the N- or C-terminus of a non-conserved range (distal disulfide), which functions to transfer electrons from reduced Mia40 or equivalents to the redox active-site disulfide, thus also referred to as shuttle disulfide [13–16]. The cysteine motif of the distal (shuttle) disulfide is highly variable phylogenetically, varying from CRXC at the N-terminus of Erv1 and ALR, CX4C at the N-terminus of PfErv (Plasmodium falciparum Erv), to CXC, CX3C and CX4C at the C-terminus of Erv2, LtErv (Leishmania tarentolae Erv) and AtErv1 respectively (Figure 1). Also, the enzyme architecture of Kinetoplastida ERV homologues (e.g. LtErv) is slightly altered with an additional C-terminal domain of ~200 amino acids with unknown function . Several structures from the core domain of ERV/ALR proteins are available, all of which crystallized as head-to-tail homodimers [17–20]. Each subunit contains a four-helical bundle that harbours the FAD cofactor and an additional (fifth) single-turn helix.
Schematic sequence alignment of ERV/ALR homologues
The interaction between Mia40 and Erv1/ALR remained unclear until a study revealed that ALR shares the same Mia40 hydrophobic binding cleft with Mia40 substrate proteins . Consistently, a recent study based on a full-length Erv1C30S/C133S mutant showed the presence of an amphipathic helix close to the shuttle cysteine residue and that it was important for the recognition of Mia40 . The current model for the Erv1 enzyme mechanism is that Erv1 oxidizes the reduced Mia40 CPC motif through the N-terminal Cys30–Cys33 shuttle disulfide, which is then reoxidized by transferring two electrons to the proximal active-site Cys130–Cys133 disulfide, and then the electrons are relayed to cytochrome c or molecular oxygen through the bound FAD for regeneration of Erv1 activity [13,22–26].
However, it was unclear how exactly the two shuttle cysteine residues (Cys30 or Cys33) of Erv1 relay electrons from the Mia40 CPC motif to the active-site disulfide. Which cysteine residue of Erv1 forms the intermolecular disulfide bond with Mia40 and whether they play overlapping or different roles in the enzymatic function are questions still remaining to be addressed. For human ALR, a gel-based analysis showed that both shuttle cysteine residues interacted equally well with the second cysteine residue of the hMia40 CPC motif , indicating that both shuttle cysteine residues have an overlapping function. On the other hand, based on the structure, the 2nd shuttle cysteine residue (analogous to Erv1 Cys33) of ALR was proposed to interact preferentially with hMia40 since it is closely followed by a stretch of hydrophobic residues responsible for substrate binding . In yeast, in the case of Erv2, it was shown that both shuttle cysteine residues were required for its function in vivo, and both single cysteine mutants can form a disulfide bond with the active-site cysteine . In the case of Erv1, although Cys33 is essential for cell viability, Cys30 seems dispensable under certain conditions [23,28]. Thus Cys33 of Erv1 was proposed to form an intermolecular disulfide bond with Mia40.
In the present study, using a combination of in vivo, in organelle and in vitro methods, we showed that both shuttle cysteine residues of Erv1 are essential for its function. They are both required for yeast cell growth, mitochondrial import of MIA substrates and Erv1 oxidase activity in the in vitro-reconstituted Mia40–Erv1 systems. Furthermore, our results showed that the two shuttle cysteine residues of Erv1 are functionally distinct; whereas Cys30 interacts and receives electrons directly from the Mia40 CPC motif, Cys33 transfers electrons gained through Cys30 to the active-site disulfide via formation of a Cys33–Cys130 intermediate disulfide bond. We also showed that Cys30 and Cys33 of Erv1 have the same pKa values and thus similar nucleophilicity despite their distinct roles in the enzymatic mechanism. Our results are consistent with the view that steric restrictions play a crucial role in thiol–disulfide exchange reactions, which mediate the kinetics and substrate specificity of the thiol oxidase enzymes.
Cloning and mutagenesis
A construct encoding C-terminally LE(H)6-tagged full-length WT (wild-type) Erv1 cloned into Escherichia coli expression vector pET24a(+) (Novagen) using the Nde1 and Xho1 restriction sites was used as DNA template  to generate all mutant constructs for protein purification work in the present study. For yeast studies, ERV1 together with endogenous promoter and terminator regions were amplified by PCR from the genomic DNA of the WT CY4 strain , followed by insertion into centromeric plasmids pRS413 and pRS414 via the Xho1 and BamH1 restriction sites. Cysteine-to-serine mutations were introduced by PCR site-directed mutagenesis (Stratagene) using overlapping primer pairs containing the desired mutation point(s). Correct sequences of all WT and mutant constructs were verified by DNA sequencing.
A S. cerevisiae strain harbouring the ERV1 gene under the GAL10 promoter  was transformed with TRP1 (tryptophan requiring 1)-containing plasmids pRS414 with or without WT Erv1 or cysteine mutants. The strains were grown on a synthetic selective medium containing glycerol (3%) supplemented with glucose (0.2%) or galactose (0.2%) in order to repress or induce the chromosomal ERV1 allele. The strains were first grown in the presence of galactose, and then shifted to a medium containing glucose for 48 h before spotting on to agar medium contai-ning glucose. For plasmid shuffling tests, a ∆erv1-knockout strain containing a copy of WT ERV1 on the URA3 plasmid  was co-transformed with the HIS3 plasmid pRS413 with or without WT or mutant ERV1 and TRP1 plasmid pRS414 with mutant ERV1. Following selection, the strains were analysed on 5-fluoro-orotic acid plates to counterselect against WT ERV1 on URA3-containing plasmid. Plates were incubated for up to 3 days at 25°C, 30°C or 37°C.
WT Erv1 and cysteine residue mutants were expressed in the E. coli strain Rosetta-gami™ 2 (Novagen). The procedure for LE(H)6-tagged protein purification was as described previously . Briefly, protein expression was induced in the presence of 0.5 mM IPTG and 10 μM FAD at 16°C for 16–20 h. The induced cell pellets were resuspended in buffer A [150 mM NaCl and 50 mM Tris/HCl (pH 7.4)] supplemented with 5 mM imidazole, 50 μM FAD and one tablet of EDTA-free protease inhibitor cocktail (Roche) and then sonicated on ice. The supernatant fraction was loaded on a column containing 2–3 ml of Ni2+-charged His. Bind resin (Novagen) pre-equilibrated with binding buffer. The column was washed with 20–30 ml of wash buffer (buffer A containing 20 mM imidazole) before the protein was eluted with 4–6 ml of elution buffer (buffer A containing 500 mM imidazole). Eluted proteins were supplemented with 100 μM FAD and stored in −80°C until further use. For GST-tagged Mia40c (amino acids 284–403), the purification procedure was as described previously . Briefly, protein was bound to 2–3 ml of glutathione–Sepharose 4B beads (GE Healthcare) overnight with gentle rotation at 4°C in buffer A. Unbound materials were removed by washing the beads with 20–30 ml of ice-cold buffer A. Protein elution was achieved by overnight incubation at 4°C in 4–6 ml of cleavage buffer (20–25 units/ml thrombin in buffer A) to remove the GST tag. All affinity-purified proteins were further purified by size-exclusion chromatography using a Superdex 75 10/30 column connected to an ÄKTA FPLC system (GE Healthcare) at 4°C in buffer A.
The PGAL-ERV1 strains were grown in liquid selective medium containing glycerol (3%) and glucose (0.2%) for 48–72 h with aeration at 30°C. Mitochondria isolation was performed as described previously .
Protein steady-state level and submitochondrial localization analyses
Total mitochondrial proteins were separated on Tris/Tricine SDS/PAGE  before Western blotting and immunodecoration with antibodies against the respective protein of interest. For protein submitochondrial localization, mitochondria (50 μg) were treated with proteinase K (0.2 mg/ml) in the presence of SM buffer [0.6 M sorbitol and 20 mM MOPS (pH 7.4)], hypotonic buffer [20 mM MOPS (pH 7.4)] or lysis buffer [1% (w/v) digitonin and 20 mM MOPS (pH 7.4)] as described in . Proteolysis was inhibited by 4 mM PMSF. Samples were TCA (trichloroacetic acid)-precipitated before analysis by Tris/Tricine SDS/PAGE (16% gel) and Western blotting.
In vitro redox time course reactions were quenched using IAM (iodoacetamide; 20 mM) or AMS (4-acetamido-4′-maleimidylstilbene-2,2′-disulfonic acid; 5 mM). For mitochondrial samples, protein thiols were alkylated with mmPEG24 (methyl-PEG24-maleimide; 2 mM). The thiol alkylation agents were prepared in 2× non-reducing SDS/PAGE sample buffer and mixed with an equal volume of protein samples at the designated time points or added to TCA-precipitated protein pellets. Samples were incubated in the dark for 30–60 min at room temperature (20°C) before resolving by Tris/Tricine SDS/PAGE (16% gel). For redox state analysis in vivo, cells were grown in glucose or galactose medium until the mid-exponential phase before incubation with 25 mM NEM (N-ethylmaleimide) to alkylate protein thiols in situ on ice for 30 min. Total cellular protein was extracted then using non-reducing SDS/PAGE sample buffer and glass beads, and separated by SDS/PAGE (16% gel) followed by Western blot analysis.
Oxygen consumption assays
Erv1 oxidase activity was measured using a Clark-type oxygen electrode (Hansatech Instrument) in a 0.5 ml reaction volume at 25°C in buffer A containing 1 mM EDTA as described previously . Data analysis of the oxygen consumption profile and the calculation of reaction slope were performed using the Microcal™ Origin™ statistical software package.
Determination of protein thiol pKa values
The pKa values of protein thiols were measured by reaction with mBBr (monobromobimane) and fluorescence detection as described in . Buffers of constant ionic strength (I=0.15 M) independent of the pH at which they are used, as proposed in , were chosen. Two buffer systems with the pH range of 3.5–9.0 (15 mM acetic acid, 15 mM Mes and 30 mM Tris) and 5.7–10 (30 mM Aces, 15.6 mM Tris and 15.6 mM ethanolamine) were used. Both buffer systems also contained 120 mM NaCl and 0.1 mM DTPA (diethylenetriaminepenta-acetic acid). Purified proteins were buffer-exchanged to their respective buffer systems using NAP-5 columns (GE Healthcare) and adjusted to the desired pH values by using variable amounts of HCl or NaOH. The reactions were started by adding mBBr (2 μM) to protein solutions (2 μM) in total reaction volumes of 125 μl. The fluorescence intensity value change was monitored at λex=396 nm and λem=482 nm for 30 min at 25°C using a Cary Eclipse fluorescence spectrophotometer. The initial rate of reaction was calculated using the points of at least the first 10 min of the reaction.
Absorption spectra were measured using a Cary 300 spectrophotometer at 1-nm intervals from 250 to 700 nm and 1 cm quartz cells at 25°C as described in . For multi-angle laser light scattering, protein samples were applied to a Superdex 200 10/30 gel-filtration column (GE Healthcare) running with buffer A. Proteins eluting from the column passed through an in-line DAWN EOS laser photometer set at 682 nm and an Optilab rEX refractor. To calculate the weight-averaged molecular mass, the light scattering intensity and eluent refractive index were analysed using ASTRA version 4.8 software.
RESULTS AND DISCUSSION
Both the shuttle cysteine residues of Erv1 are required for cell viability
To investigate the requirement of individual shuttle cysteine residues of Erv1 in the protein function in vivo, we checked the cell viability by expressing plasmid-encoded Erv1 single cysteine-to-serine (C30S and C33S) mutants, hereafter named Erv1SXXC and Erv1CXXS, in the ERV1-knockout strain ∆erv1 that is isogenic to the WT W303  (see the Experimental section; Figure 2). Upon counter-selection of WT ERV1 on the URA3-containing plasmid, both mutants were unable to support cell growth at 30°C, suggesting that both Cys30 and Cys33 are required for yeast cell growth and thus the function of Erv1. Furthermore, co-expression of Erv1SXXC and Erv1CXXS also failed to rescue cell viability (Figure 2), indicating that these cysteine residues do not interact in trans, as they are required to be in the same CXXC motif in order to function. Our observation was different to the result previously published  where it was observed that only Erv1CXXS was lethal and there was a WT-like cell growth at 30°C for Erv1SXXC using the pYX142 overexpressing plasmid and a ∆erv1-knockout strain derived from the same genetic background. We did not observe any cell growth for Erv1SXXC when the experiment was carried out at 25°C either (results not shown). It is probable that the discrepancy observed in the Erv1SXXC complementation experiments between the present study and the one described previously  is due to the plasmid used and expression level of the protein. In the present study, the ERV1 mutant was cloned in the centromeric plasmid pRS413, together with the endogenous promoter and terminator region. In , the mutant was cloned in pYX142 that is also a centromeric vector, but under the control of the promoter of the TPI1 (triose phosphate isomerase 1) gene, encoding the abundant glycolitic enzyme Tpi1. Based on the global analysis of protein expression in yeast , Tpi1 protein level was estimated to be more than 2.07×105 molecules/cell, whereas the Erv1 level was not detectable, meaning below the detection limit of 50 molecules/cell. Thus, under the control of the strong TPI1 promoter, Erv1SXXC may act as a multicopy suppressor of the Δerv1 growth-deficient phenotype, and can rescue the cell viability when it is overexpressed at a non-physiologically high level. In summary, our results suggest that both N-terminal shuttle cysteine residues of Erv1 are required for cell viability and. hence. Erv1 function providing that the mutant proteins were correctly imported into the mitochondria.
Both the N-terminal cysteine residues of Erv1 are required for cell viability
The shuttle cysteine mutants of Erv1 are localized in the mitochondrial IMS
Since we observed both mutants Erv1SXXC and Erv1CXXS not being able to support cell growth, we checked whether the mutation of the shuttle cysteine residues resulted in defective import of Erv1 into the mitochondria. To achieve this, we used a yeast strain with ERV1 gene under the control of a GAL10 promoter  transformed with plasmids encoding for WT or mutant Erv1 (Figure 3a). A strain with the empty vector (−) was used as a background control. Upon depletion of endogenous Erv1 in the presence of glucose, although the strain with plasmid-encoded WT Erv1 showed a normal growth phenotype, mutation of either one or both shuttle cysteine residues induced a cell growth defect as that observed for the background control strain at 30°C (Figure 3a). The low background level growth was probably due to a very low level of endogenous Erv1 which was sufficient to support growth. A similar result was observed at an elevated temperature of 37°C. At 37°C, there was a more pronounced growth defect for all the mutant and background control strains, whereas the growth of the WT strain was unaffected (results not shown). Thus these results are consistent with those obtained from using the ∆erv1-knockout strain (Figure 2), suggesting that both the N-terminal shuttle cysteine residues of Erv1 are required for cell growth.
Mutation of the N-terminal cysteine residues had no effect on Erv1 localization in the mitochondrial IMS
The PGAL-ERV1 strains carrying the Erv1 mutant plasmids allowed cell growth to a certain extent under the condition tested due to a very low undetectable level of endogenous Erv1 (see Figure 4a, lane -). This enabled us to isolate the mitochondria from the strains for further analyses. To check Erv1 localization in the mitochondria, we tested the proteolysis susceptibility of Erv1 and mitochondrial marker proteins in each of the mitochondrial subcompartments (Figure 3b). Tom40 (translocase of the outer mitochondrial membrane 40 kDa), cytochrome b2 and Cpn10 (chaperonin 10) were used as marker proteins in the mitochondrial OM (outer membrane), IMS and matrix respectively. Like cytochrome b2, the WT and mutant Erv1 proteins were detectable in intact mitochondria (Mito) but susceptible to protease diges-tion in mitoplasts (M.P.) when proteinase K was present (Figure 3b, lanes 1–4), indicating that the proteins were successfully imported into the mitochondrial IMS. Thus the shuttle cysteine mutations had no obvious effect on Erv1 localization, which is consistent with the observations that shuttle cysteine mutants had mild effects on the in vitro import of Erv1 [23,39].
Mutation of the shuttle cysteine residues of Erv1 affected the function of MIA pathway
In conclusion, yeast complementation assays and mitochondrial protein localization analyses show that both of the N-terminal shuttle cysteine residues are required for cell growth and thus the function of Erv1.
Both of the N-terminal shuttle cysteine residues are required for the import of MIA substrates in vivo
After establishing the requirement of both Cys30 and Cys33 for Erv1 function, we then asked whether they are both required for the import of MIA substrates by checking the steady-state levels of proteins in the mitochondria isolated from the strains with depleted endogenous Erv1 (Figure 4a). In agreement with our results from the in vivo complementation assays, the protein level of MIA substrates (small Tim proteins and Erv1), which are essential for cell growth, was significantly decreased in mitochondria containing Erv1 with either one or both of the N-terminal shuttle cysteine residues mutated compared with that of the WT. As controls, the steady-state levels of other mitochondrial proteins were unaffected. These results indicated that the defect in the MIA pathway may be due to a functional defect of Erv1 mutants. However, we cannot conclude whether the effects were exclusively due to the cysteine mutations or to a combination of Erv1 abundance and compromised enzyme function.
To demonstrate the effect of the cysteine mutations on the MIA pathway more directly, we analysed the redox state of the Mia40 CPC motif in the mitochondria containing WT and mutant Erv1 (Figure 4b). In the presence of WT Erv1, more Mia40 (approximately 43%) was in an oxidized state (lane 5) compared with approximately 25% oxidized Mia40 in the mitochondria from the empty vector (lane 4) and mutant Erv1 strains (lanes 6–8), suggesting that the mutants had defects in oxidizing Mia40. Furthermore, we analysed the cysteine-redox state of Mia40 in vivo using whole cell extracts with NEM alkylation (Figure 4c) as described previously . Consistently, upon depletion of endogenous Erv1 by growing the cells in glucose medium, approximately 50% Mia40 from the WT Erv1 strain was oxidized, but most of the proteins were reduced (~80%) in cells containing the empty vector or mutant Erv1 (Figure 4c, lanes 4–8). On the other hand, the same redox state distribution was observed for all strains when they were grown in galactose medium (lanes 9–13) when endogenous Erv1 was overexpressed. Western blot analysis of Erv1 showed that the same level of endogenous Erv1 was overexpressed in galactose medium. When the cells were grown in glucose medium, Erv1 was not detectable due to a low level of Erv1 expression .
Taken together, our findings suggest that both Cys30 and Cys33 are essential for Erv1 function in the MIA pathway, which is ultimately required for cell viability.
Cys33 is involved in transferring electrons to the redox centre
To understand why both the shuttle cysteine residues are vital for Erv1 function, we investigated the function of individual cysteine residues in vitro using the recombinant single cysteine mutant proteins Erv1SXXC (Erv1C30S) and Erv1CXXS (Erv1C33S) expressed and purified from E. coli cells (see the Experimental section). Although purified Erv1CXXS was yellowish as with the WT and the corresponding double cysteine mutant Erv1SXXS , Erv1SXXC was a black colour as reported previously . We analysed the proteins further using gel-filtration chromatography (Figure 5a). Erv1SXXC (C30S) eluted into two main peaks (black curve). Then, the molecular masses of the fractions were determined by light-scattering analysis to be approximately 99.8 kDa (peak 1) and 48.7 kDa (peak 2) respectively, suggesting that this mutant existed as both a tetramer and a dimer. Interestingly, the two peaks showed different colours, a WT-like yellow for peak 1 and black for peak 2. For Erv1CXXS (C33S), two partially overlapping peaks were obtained eluted at the void volume (higher oligomers) and the position corresponding to the Erv1 tetramer (Figure 5a, grey curve).
Characterization of purified Erv1 mutant proteins
UV–visible spectroscopy analysis (Figure 5b) revealed that both the yellowish species (peak 1) of Erv1SXXC (C30S) and Erv1CXXS (C33S) had a very similar spectra profile as that of the WT with a bound FAD absorbance at 460 nm. However, the black species (peak 2) of Erv1SXXC (black curve) had a scattered increasing absorbance at the visible spectrum with a broadened peak at ~447 nm and an additional peak at ~580 nm, which is an indication of the presence of an S−-FAD CTC (charge-transfer complex) as reported previously . Upon treatment with the reducing agent TCEP [tris-(2-carboxyethyl)phosphine], the spectra profile changed to the WT-like spectrum (Figure 5b, dotted curve), indicating that the intermediate CTC was resolved. We reasoned that the black-coloured Erv1SXXC represents a charge-transfer intermediate containing a trapped disulfide bond between Cys33 and Cys130 of the active-site disulfide, leaving the unpaired Cys133 to form an S−-FAD CTC as seen in several flavoenzymes [16,28,40,41]. Upon TCEP treatment, the Cys33–Cys130 disulfide bond and the CTC were resolved, and the subsequent formation of the active-site Cys130–Cys133 disulfide bond led to the appearance of a WT-like absorption spectrum. No CTC was detected in Erv1CXXS, suggesting that it is unlikely for Cys30 to interact directly with the active-site disulfide bond. Thus Cys33 is functionally distinct from Cys30 in relaying electrons to the redox centre.
Cys30 of Erv1 is more reactive in inter-molecular disulfide bond formation
The gel-filtration analysis (Figure 5a) showed that Erv1CXXS, in the presence of Cys30, was prone to form higher-molecular-mass oligomers, and the relative amount of the oligomers decreased significantly upon mutation of Cys30 in both the single and double mutants. This result suggested that Cys30 may be more solvent exposed and plays a more prominent role than Cys33 in forming the intermolecular disulfide bond. To test this, we analysed the gel-filtration fractions of the purified proteins using reducing and non-reducing SDS/PAGE (Figure 6a). As predicted, the results showed that all of the fractions of Erv1CXXS were dominated by an intermolecular disulfide-bonded dimer and more prone to form such a dimer than Erv1SXXC. Such a dimer band was observed for the WT, redox active-site and struc-tural disulfide double cysteine mutants (C130/C133S and C157/C176S), but not detectable or negligible for the double shuttle cysteine mutant (C30/C33S) (Supplementary Figure S1 at http://www.biochemj.org/bj/460/bj4600199add.htm), suggesting that the dimer band in Figure 6(a) contained mainly Erv1 dimers linked via Cys30–Cys30′ or Cys33–Cys33′ intermolecular disulfide bond respectively. Thus the higher reactivity of Cys30 compared with that of Cys33 for intermolecular disulfide bond formation between Erv1 molecules gave an early indication that Cys30 may play an important role in receiving electrons from protein thiols of substrate molecules.
Cys30 is more reactive than Cys33 for intermolecular disulfide bond formation
Next, to understand whether Cys30 of Erv1 is more reactive than Cys33 in interacting with the Mia40 CPC motif, Erv1SXXC and Erv1CXXS were incubated with single cysteine mutants of the core domain Mia40 (~15 kDa; see the Experimental section) CPC motif disulfide (hereafter named Mia40SPC and Mia40CPS) respectively, in all four possible combinations and then analysed using non-reducing SDS/PAGE. Although an adduct of the ~37 kDa band was observed in all four combinations (Figure 6b, lanes 3, 4, 9 and 10), Erv1CXXS plus Mia40SPC showed the most intensive band (lane 9). This adduct was dissociated under reducing conditions (Figure 6b, lanes 5, 6, 11 and 12), showing that the 37 kDa adduct was an Mia40–Erv1 complex containing an intermolecular disulfide bond between the mutant proteins (15 kDa Mia40 and 22 kDa Erv1). The highest amount of the complex was detected in the mixture of Erv1CXXS and Mia40SPC (Figure 6b, lane 9), implying that the mixed disulfide formed between the first cysteine residue (Cys30) of Erv1 and the second cysteine of the Mia40 CPC motif is the most favourable. This result was confirmed and shown more clearly by time course analyses (Figure 6c). The complex formed between of Erv1CXXS (Cys30) and Mia40SPC was most prominent and effective compared with the other three combinations (Figure 6c, lanes 2–5). Taken together, our results suggest that Cys30 is more reactive than Cys33 in forming an intermolecular disulfide bond with Mia40, and more reactive towards the second cysteine residue of Mia40 CPC.
In human ALR, however, this was not the case, as both of its shuttle cysteine residues had an equal level of interaction with the second cysteine of the hMia40 CPC motif based on cysteine mutation and non-reducing gel analyses . Furthermore, detailed structural characterization of the ALR–hMia40 covalent adducts suggested that the second shuttle cysteine residue of ALR (analogous to Erv1 Cys33 rather than Cys30) may interact preferentially with hMia40 attributed to the presence of hydrophobic residues downstream of the second shuttle cysteine residue (bold) of ALR (CRACVDFKTWM) . Similar, but different, hydrophobic residues are present downstream of Erv1 Cys33 (bold) (CRSCNTLLDFQ). A previous computational simulation suggested that Cys33 of Erv1 may form an intermolecular disulfide bond with Mia40 driven by hydrophobic interactions . It is worth to mention that the domains containing the shuttle cysteine residues of Erv1 and ALR are not conserved and both are largely unstructured. A recent structural study has suggested that the shuttle cysteine residues of Erv1 and ALR have different structural and solvent exposal properties . Although both shuttle cysteine residues of ALR are located in a flexible segment, Cys33 of Erv1 seems to be part of a α-helical structure with Cys30 unstructured and thus more solvent exposed . This result is consistent with our observation that Cys30 is more reactive than Cys33 in forming intermolecular disulfide bond between Erv1–Erv1′ and with Mia40.
Next, we asked whether the higher reactivity of Cys30 of Erv1 is due to the fact that it has a lower pKa value than Cys33. In order to determine the pKa of both shuttle cysteine residues of Erv1, we generated two triple cysteine mutants from the single cysteine mutants Erv1CXXS and Erv1SXXC, in which both active-site cysteine were mutated to serine (named as Erv1CSSS and Erv1SCSS) to avoid potential thiol–disulfide exchange reactions. AMS thiol-modification confirmed that both Cys30 and Cys33 were reduced and accessible to a thiol alkylating agent (Figure 7a). Time courses of the interaction of the triple mutant with mBBr combined with fluorescence detection were measured at various pHs and the initial rates were determined. As a control, the redox active-site disulfide mutant Erv1CCSS with the shuttle cysteine residues oxidized (Figure 7a, lane 2) was used. The results showed that both Cys30 and Cys33 have the same apparent pKa values of 8.4±0.1 (Figure 7b). Thus the higher reactivity of Cys30 than that of Cys33 for disulfide bond formation was not due to a low pKa.
pKa determinations for Cys30 and Cys33 of Erv1
Both Cys30 and Cys33 of Erv1 are required for enzyme turnover
To understand further whether and why both Cys30 and Cys33 are required for the oxidase activity of Erv1, we analysed the oxidase activity of Erv1 mutants using gel-based AMS thiol modification and oxygen consumption assays using purified reduced Mia40 as a substrate . First, as shown in Figure 8(a), Mia40 was fully oxidized within 2 min of incubation with the WT Erv1 (lanes 6–8). However, Mia40 stayed in a reduced form throughout the time course when incubated with Erv1SXXC and Erv1CXXS respectively (Figure 8a, lanes 9–14), or with both mutants together (lanes 15–17). Next, Erv1 activity was measured by oxygen consumption (Figure 8b). Consistently, only the WT Erv1 was able to catalyse the electron transfer from Mia40 to molecular oxygen, but not the mutants alone or in a combination. These results showed that both Cys30 and Cys33 are required, and must be in the same CXXC motif (not CXXS+SXXC) for Erv1 enzyme activity turnover.
Both of the shuttle cysteine residues are required for oxidase function of Erv1
Theoretical and computational studies have suggested that the thiol–disulfide exchange reaction proceeds through a SN2 transition state, and steric restriction plays a significant role in such a reaction [43,44]. The thiol–disulfide exchange reaction proceeds optimally when the attacking thiolate and the disulfide bond are in a co-linear position [43,44]. Consistently, our results showed that Cys30 of Erv1 in the same CXXC motif with Cys33 is essential for Erv1 enzyme activity. We reasoned that Cys30 is required for the intermediate disulfide Cys33–Cys130 to be resolved rapidly allowing the active enzyme be regenerated effectively. Taken together, these results showed that both shuttle cysteine residues are required for Erv1 oxidase activity and provided an explanation why both the single shuttle cysteine mutations caused cell growth defect (Figures 2 and 3a).
In the present study, we have shown that both shuttle cysteine residues of Erv1 are required for Erv1 function and that they each play distinct roles in the Mia40–Erv1 enzymatic mechanism. Together with the results of previous studies [13,17,28], we propose a model for Erv1 thiol–disulfide exchange reactions with a focus on the reductive half-reaction (Figure 9). Cys30 of Erv1 is much more reactive than Cys33 in forming an intermolecular disulfide bond with the second cysteine residue of the Mia40 CPC motif, thus Cys30 is the preferred cysteine to interact directly with Mia40 in the Mia40–Erv1 reaction. In the Erv1–Erv1′ electron transfer reaction, Cys33 is essential for forming the intermediate disulfide Cys33–Cys130′ (where Cys130′ is the interchange cysteine of another subunit), whereas Cys30 is required for resolving the intermediate disulfide for efficient turnover of the enzyme. We propose that Cys30 of Erv1 plays two important roles: interacting with Mia40 and resolving the Erv1 intermediate disulfide Cys33–Cys130′ effectively. Taken together, both shuttle cysteine residues of Erv1 are required for its function, and they play complementary, but distinct, roles to ensure rapid turnover of Erv1 enzyme activity both in vivo and in vitro. In addition, the higher versatility of shuttle cysteine motifs and domains, and different levels of functional specificity between the shuttle cysteine residues in ERV/ALR enzymes highlight an evolutionary divergence of ERV/ALR homologues.
Model of thiol–disulfide exchange reactions in Erv1 catalysis
augmenter of liver regeneration
Arabidopsis thaliana Erv1
cytochrome c oxidase 17
essential for respiration and viability
Leishmania tarentolae Erv
mitochondrial import and assembly
Plasmodium falciparum Erv
translocase of the inner membrane
triose phosphate isomerase 1
tryptophan requiring 1
Swee Kim Ang and Hui Lu designed the research; Swee Kim Ang and Mengqi Zhang performed the experiments; Swee Kim Ang, Mengqi Zhang and Hui Lu analysed the data; Tiziana Lodi generated the erv1-deletion yeast strain; and Swee Kim Ang and Hui Lu wrote the paper with contribution from Tiziana Lodi.
We thank the faculty biomolecular analysis core facility for help with light scattering measurement, Michael Spiller for advice on yeast genetics and reading the paper before submission, and Professor Kai Hell (Ludwig Maximilians University Munich, Munich, Germany) and Dr Jan Riemer (TU Kaiserslautern, Kaiserslautern, Germany) for the PGAL-ERV1 yeast strain and anti-Erv1 antibody respectively.
This work was supported by the Biotechnology and Biological Sciences Research Council [grant number BB/H017208] and the Leverhulme Trust [grant number F/00120/CB].