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Article

Methionine Sulfoxide Reductases Contribute to Anaerobic Fermentative Metabolism in Bacillus cereus

by
Catherine Duport
1,*,
Jean-Paul Madeira
1,
Mahsa Farjad
1,
Béatrice Alpha-Bazin
2 and
Jean Armengaud
2
1
Département de Biologie, Avignon Université, INRAE, UMR SQPOV, F-84914 Avignon, France
2
Département Médicaments et Technologies pour la Santé (DMTS), Université Paris-Saclay, CEA, INRAE, SPI, F-30200 Bagnols-sur-Cèze, France
*
Author to whom correspondence should be addressed.
Antioxidants 2021, 10(5), 819; https://0-doi-org.brum.beds.ac.uk/10.3390/antiox10050819
Submission received: 2 April 2021 / Revised: 16 May 2021 / Accepted: 17 May 2021 / Published: 20 May 2021
(This article belongs to the Special Issue Redox Biology in Microorganisms)
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Abstract

:
Reversible oxidation of methionine to methionine sulfoxide (Met(O)) is a common posttranslational modification occurring on proteins in all organisms under oxic conditions. Protein-bound Met(O) is reduced by methionine sulfoxide reductases, which thus play a significant antioxidant role. The facultative anaerobe Bacillus cereus produces two methionine sulfoxide reductases: MsrA and MsrAB. MsrAB has been shown to play a crucial physiological role under oxic conditions, but little is known about the role of MsrA. Here, we examined the antioxidant role of both MsrAB and MrsA under fermentative anoxic conditions, which are generally reported to elicit little endogenous oxidant stress. We created single- and double-mutant Δmsr strains. Compared to the wild-type and ΔmsrAB mutant, single- (ΔmsrA) and double- (ΔmsrAΔmsrAB) mutants accumulated higher levels of Met(O) proteins, and their cellular and extracellular Met(O) proteomes were altered. The growth capacity and motility of mutant strains was limited, and their energy metabolism was altered. MsrA therefore appears to play a major physiological role compared to MsrAB, placing methionine sulfoxides at the center of the B. cereus antioxidant system under anoxic fermentative conditions.

Graphical Abstract

1. Introduction

Bacillus cereus is a notorious food-borne gram-positive pathogen that can adapt to various oxygenation conditions encountered in the environment, in foods and in the human intestine [1]. Under anaerobiosis and in the absence of a final electron acceptor such as nitrate, B. cereus sustains its growth by producing ATP through mixed acid fermentation. This process generates lactate as the main metabolite, along with smaller amounts of acetate, formate, succinate, and ethanol [2,3,4]. Traditionally, fermentative conditions are not considered to produce reactive oxygen species (ROS), due to the decreased oxidative phosphorylation taking place. However, experimental evidence suggests that an antioxidant response nevertheless occurs in fermenting B. cereus cells [5,6]. This response may be due to B. cereus undergoing transient secondary oxidative stress upon exposure to anaerobic fermentative conditions, through nitric oxide (NO) production [7], as a result of the action of nitric oxide synthase on arginine [8,9,10].
The sulfur-containing methionine residues in proteins are especially sensitive to ROS-mediated oxidation [11]. Oxidation of methionine results in two diastereomic forms of methionine sulfoxide (Met(O)): methionine-S-sulfoxide (Met-S-O) and methionine-R-sulfoxide (Met-R-O). The reaction is reversible thanks to the action of methionine sulfoxide reductase (Msr) [12]. Four types of Msr have been identified that reduce Met(O) residues to their functional form [13]. The main types are the thiol-oxidoreductases MsrA and MsrB, which react specifically with diastereomers displaying the S- and R-configurations at the sulfur atom, respectively [14,15]. The third and fourth types of Msr belong to the molybdenum-containing enzyme families. The third type of Msr, periplasmic methionine sulfoxide reductase (MsrP), is present in most gram-negative bacteria and is a member of the sulfite oxidase family. MsrP is not a stereospecific protein-MetO reductase [16]. The fourth type of Msr belongs to the dimethyl sulfoxide (DMSO) reductase family. One example is the periplasmic Rhodobacter sphaeroides DorA DMSO reductase, which reduces DMSO and both free and protein-bound Met-S-O [13]. The primary role of the first three types of Msr is to regulate the Met(O) level in proteins; they reduce Met(O) residues more efficiently in unfolded proteins than in folded proteins [17]. The role of DorA-like enzymes in protecting proteins against oxidation remains to be validated in vivo [16]. Cyclic Msr-dependent methionine oxidation/reduction was proposed to be an important antioxidant defense mechanism in both bacteria and eukaryotic cells, playing a scavenging role for cellular ROS under normal and stressed conditions [11,17,18,19,20]. Msr can also regulate protein function by modulating specific Met(O) residues involved in protein activation or inactivation [21]. Consequently, these enzymes are implicated in a variety of biological processes, including redox signaling, cellular metabolism, and virulence. Although Msr and other antioxidants have been identified in both facultative and strict anaerobes [22,23], their role in cellular processes under anoxic conditions remains largely uncharacterized. The few studies available report results for yeast, where MsrA and MsrB were reported not to contribute to the ROS-regulated lifespan under strict anoxic conditions [24], and for the strict anaerobic bacterium Clostridium oremlandii, where high activity levels of the selenoprotein MsrA were detected [25]. However, no physiological role has yet been proposed for these enzymes in anoxic conditions.
Whole-genome sequence analysis of B. cereus ATCC 14579 revealed two genes encoding Msr. The first of these genes, msrAB, encodes a bifunctional cytoplasmic MsrAB enzyme, and is probably the result of gene fusion [26]. Our previous results indicated that MsrAB plays a key role in redox homeostasis in B. cereus under aerobic respiratory conditions, and regulates exotoxin secretion [27]. The role of MsrA has not been investigated to date. For this study, we generated single and double mutants of msrA and msrAB to investigate the antioxidant role of Msr proteins, under anaerobic fermentative growth conditions, using a proteomics approach. The results suggest that the repair of Met(O)-containing proteins contributes significantly to anaerobic fermentative growth of B. cereus, and demonstrate clearly distinct in vivo contributions from MsrA and MsrAB to the reduction of cellular protein-bound Met(O).

2. Materials and Methods

2.1. Strains, Media, and Growth Conditions

Wild-type B. cereus ATCC 14579 without its pBClin15 plasmid [28], the single mutants ΔmsrA, ΔmsrAB [27], and the ΔmsrAΔmsrAB double mutant strains were grown either in Luria broth (LB) or MOD medium supplemented with 30 mM glucose (MODG) as the carbon source, as previously described [3]. Controlled anaerobic batch cultures were performed at 37 °C in 2 L bioreactors (Discovery 100, Iceltech, France) containing 1.5 L MODG medium. pH was maintained at 7.2 by automatic addition of 5 M KOH, and constant shaking at 300 rpm. Anaerobiosis (pO2 = 0%) was obtained by continuously flushing the medium with pure nitrogen gas (20 mL/h) that had been passed through a Hungate column. The inoculum was a 100-mL sample of an exponential anaerobic culture (250 mL Erlenmeyer flasks fitted with open-top caps and rubber septa) harvested by centrifugation, washed twice and diluted in fresh MODG medium to obtain an initial optical density at 600 nm of 0.02. Three biological replicates were analyzed for each strain.

2.2. Analytical Procedures

The growth of B. cereus WT and mutant strains was monitored spectrophotometrically at 600 nm. The maximal specific growth rate (µmax) was determined by applying the modified Gompertz equation [29]. Culture samples (250 mL) were harvested anaerobically during the early exponential (EE, µ= µmax), late exponential (LE), and stationary (S) growth phases and treated in an anaerobic chamber. Cells and culture supernatants were separated by centrifugation (10,000× g, 10 min, 4 °C). Cells were suspended in PBS buffer, and stored at −20 °C. Supernatants were filtered as previously described [6], aliquoted in small volumes, and stored frozen at −20 °C until analysis.
Glucose, lactate, ethanol, formate, acetate, and succinate concentrations were determined in filtered supernatants using Enzytec Fluid kits (R-Biofarm, Saint-Didier-au-Mont-d’Or, France) according to the manufacturer’s protocol.
Cellular and extracellular proteins were extracted from cell pellets and filtered supernatant samples as previously described [27,30]. All manipulations were performed in an anaerobic chamber to avoid artefactual oxidation.

2.3. Relative Quantification of msrA and msrAB Gene Expression

Real time quantitative RT-PCR experiments were performed as described previously [27]. Briefly, real-time RT-PCR was performed using the iScript™ One-Step RT-PCR kit with SYBR® Green following the manufacturer’s protocol (Biorad, Marne-La-Coquette, France), with 10 ng of total RNA as a template. Total RNA was extracted from B. cereus cells at EE, LE and S growth phases by using TRI Reagent RNA extraction solution as recommended by the manufacturer (Ambion, Thermo Fischer Scientific, Illkirch, France). The Agilent 2100 Bioanalyzer system was used to characterize and quantify total RNA. The mRNA level changes for each gene were normalized to the RNA level for the ssu gene, encoding 16S RNA, and quantified by the 2−ΔΔCT method. The specific primer pairs used in these experiments were: 5′-TTCTGGTACACAGGTGGTC-3′ and 5′-AAAGCGTCCACTCTGCTCAA-3′ for msrAB (BC_5436, NC_004722.1); 5′-TCCAACTGATGATGGCGGAC and 5′-TCACGCCCAGATTCTTTTTGC-3′ for msrA (BC_1774, NC_004722.1). Data from two technical replicates, for each of the three biological replicates, were used to conduct statistical analysis.

2.4. Construction of msrA Mutant Strains

The msrA gene (BC 1774) was disrupted in B. cereus ATCC 14579 by allelic exchange with a spectinomycin resistance cassette (SpR, [31]), and in the B. cereus ΔmsrAB strain by exchange with a kanamycin resistance cassette (KmR), as described by Arnaud et al. ([32]). Briefly, a 949-bp DNA fragment encompassing the msrA gene was obtained by PCR using the following primers: 5′GAATTCGCTTAGGTGAAGTAGAAGACATTG-3′ (with an EcoRI site at the 5′end) and 5′AGATCTGTATATAAGATGGACAATTAAACAAAG-3′ (with a BglII site at the 5′ end). The PCR product was cloned into pCRXL-TOPO (Invitrogen, Thermo Fischer Scientific, Illkirch, France), and the recombinant plasmid (pCRXL-TOPO:msrA) was digested with XmnI. The 1.5-kb SpR cassette was isolated from pDIA [2] by digestion with SmaI, and the 1.5-kb KmR cassette was isolated from pDG789 [33] by digestion with SmaI and StuI. The resistance cassettes were ligated into the XmnI-digested pCRXL-TOPO:msrA vector. The resulting plasmids were subsequently digested with EcoRI and BglII to extract the msrA::SprR and msrA::KmR fragments. These fragments were cloned into pMAD precut with the same restriction enzymes. The pMAD-msrA::SprR plasmid was introduced into B. cereus WT and the pMAD-msrA::KmR was introduced into the ΔmsrAB mutant by electroporation. The msrA gene was deleted in both strains by a double crossover event. Chromosomal allele exchanges were confirmed by PCR with oligonucleotide primers located upstream and downstream of the DNA regions used for allelic exchange. For some experiments, the msrA gene was complemented in trans by cutting the pCRXL-TOPO:msrA plasmid with EcoRI and BglII and ligating the product to similarly digested pHT304 [34]. The integrity of the insert in the recombinant vector was verified by sequencing, and the vector was then used to transform the B. cereus mutant strains.

2.5. Proteomics Analysis

Cellular and extracellular proteins from the 36 samples (3 biological replicates × 3 time-points × 4 strains) of WT, ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB strains were subjected to a short electrophoretic migration (about 3 min) on NuPAGE 4–12% Bis-Tris gels (Invitrogen, Thermo Fischer Scientific, Illkirch, France) using NuPAGE MES supplemented with NuPAGE antioxidant as running buffer [35]. Proteins were then submitted to in gel proteolysis with sequencing-grade trypsin (Roche, Sigma Aldrich, Saint Quentin Fallavier, France) according to the ProteaseMAX protocol (Promega, Madison, WI, USA) [36,37]. Samples were analyzed by Liquid Chromatography with Tandem Mass spectrometry (nanoLC-MS/MS) using an LTQ-Orbitrap XL hybrid mass spectrometer (Thermo Fisher Scientific, Illkirch, France) coupled to an Ultimate 3000 nRSLC system (Dionex, Thermo Fisher Scientific, Illkirch, France). NanoLC-MS/MS analysis was performed as previously described [27,38]. Briefly, peptides were resolved on a Dionex nanoscale Acclaim Pepmap100 C18 capillary column (3 μm bead size, 100 Å pore size, 75 μm i.d. × 15 cm) at a flow rate of 0.3 μL/min over 90 min, applying a gradient from 5 to 60% solvent B (0.01% HCOOH/100% CH3CN) and, over 180 min, applying a gradient from 5 to 50% solvent B. Solvent A was 0.01% HCOOH/100% H2O. Tryptic MS/MS spectra were searched against an in-house B. cereus ATCC 14579 database using the MASCOT Daemon search engine with the following parameters: 5 ppm peptide tolerance, 0.5 Da fragment ion tolerance, 2+ or 3+ peptide charge, a maximum of two missed cleavages, carbamidomethylation of cysteine (+57.0215) as fixed modification, and oxidation of Met (+15.5949) as a variable modification. Only peptides identified with a p-value < 0.05 in homology threshold mode, and proteins identified by at least two distinct peptides, were retained upon parsing with IRMa software v1.3.1 [39]. The false positive rate determined from the corresponding decoy database was estimated to be less than 1%.
Changes in protein abundance and Met(O)peptide levels between WT and mutant strains at the different time-points were analyzed using the Bioconductor DEP package (version 1.12.0), and R version 4.0.2 [40]. Met(O)peptides were first filtered to ensure two valid identifications in at least two biological replicates. Relative Met(O)peptide abundance levels were calculated based on the Met(O) spectral count normalized with respect to the total number of spectra. Missing values were imputed using random draws from a Gaussian distribution centered around a minimal value. Relative protein abundances were calculated based on spectral counts after correction and normalization by variance stabilizing (vsn), using the Limma package. Significant changes were selected where the adjusted p-value was less than 0.05 and the |fold-change| ≥1.5.
Mass spectrometry associated proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository under dataset identifiers PXD024888 for the cellular proteome of B. cereus ATCC 14579, PXD024927 for the cellular proteome of the ΔmsrAB mutant, PXD024850 for the cellular proteome of ΔmsrA mutant, PXD024849 for the cellular proteome of ΔmsrABΔmsrA mutant, PXD024702 for the exoproteome of B. cereus ATCC 14579, PXD024714 for the exoproteome of ΔmsrAB mutant, PXD024847 for the exoproteome of ΔmsrA mutant, and PXD024848 for the exoproteome of the ΔmsrABΔmsrA mutant.

2.6. Motility Assays

The B. cereus WT and mutant strains were grown overnight and surface-spotted (5 µL) in the center of Tryptone-NaCl plates (1% tryptone, 0.5% NaCl) semi-solidified with 0.25% and 0.7% agar to assess swimming and swarming motility, respectively [41]. Motility diameters (indicative of migration of the bacteria from the center to the periphery of the plate) were measured after 72 h incubation at 37 °C in AnaeroPack™ Jars (Thermo Fisher, Scientific, Illkirch, France). Biological triplicates were performed for all experiments.

2.7. Statistical Analyses

Data from three biological replicates were pooled for statistical analyses. Comparisons among multiple groups were analyzed by analysis of variance (ANOVA) followed by Tukey’s post hoc analysis (qRT-PCR and Met(O) quantification experiments). Changes in motility and metabolite production were evaluated using the Student’s t-test. Statistical analyses were performed using XLSTAT software (version 2021.1, Addinsoft, Paris, France). p-values ≤ 0.05 were considered significant.

3. Results

3.1. Expression Patterns for B. cereus msrA and msrAB RNA and Proteins under Fermentative Anaerobic Conditions

In silico analysis of the B. cereus ATCC 14579 genome identified two genes encoding methionine sulfoxide reductase. The first gene, msrAB (BC_5436), has been described elsewhere and encodes a cytoplasmic MsrAB protein [27]. The second gene (BC_1774) was annotated as msrA. It encodes a predicted cytoplasmic MsrA protein consisting of 178 amino acids, with a theoretical molecular mass of 20475 Da. This protein contains an MsrA domain that shares 64% sequence identity to the MsrA domain of the bifunctional MsrAB protein.
We compared the mRNA levels of msrA and msrAB during the EE, LE, and S growth phases under anoxic conditions. Figure 1 shows that maximum mRNA expression levels for msrA and msrAB were reached during the LE growth phase and, in contrast to msrAB, the mRNA level for msrA was higher during the EE growth phase than during the S growth phase (p < 0.05). The kinetics of msrAB expression under anaerobiosis was distinct from that described previously under aerobiosis [27]. Both msrA and msrAB mRNA levels increased under aerobiosis during active growth, and remained high during the stationary growth phase (Figure S1). This expression profile suggests that the growth-phase-dependent expression of msr genes is influenced by oxygenation conditions.
We next performed high-resolution tandem mass spectrometry analyses to detect MsrA and MsrAB in the B. cereus anoxic cellular proteome. Only one peptide was assigned to each of the two Msr in this analysis (data not shown). The same analysis of an oxic cellular proteome detected two and five peptides for MsrA and MsrAB, respectively [27]. No Msr-peptide was detected in B. cereus exoproteome whatever the oxygenation conditions, indicating that both MsrA and MsrAB are cytoplasmic proteins. These results suggest that both Msr proteins are expressed at low abundance, and that their levels are decreased when cells are grown in anaerobic conditions compared to aerobic growth conditions.

3.2. Effect of msrA and msrAB Mutations on Anaerobic Fermentative Metabolism

We previously reported the construction of a ΔmsrAB mutant strain [27]. For the present study, we disrupted the msrA gene in WT and msrAB mutant strains to create a single ΔmsrA mutant and a double ΔmsrAΔmsrAB mutant, respectively. Quantitative RT-PCR analyses confirmed that both mutant strains lack msrA expression. Expression was restored by complementation of these strains with a plasmid carrying the msrA gene (pHT304-msrA) (data not shown).
We first compared the growth features of the ΔmsrA, ΔmsrAB and double ΔmsrAΔmsrAB mutants to those of the parental ATCC 14579 wild-type strain (Figure 2). A similar maximal specific growth rate (µmax) was measured for all four strains (Table 1).
However, ΔmsrAΔmsrAB and ΔmsrA mutants reached the stationary growth phase at a lower final biomass than the ΔmsrAB mutant and WT strains (1.3 and 2-fold decrease, respectively, Figure 2, Table 1). Interestingly, the final biomass recorded for the ΔmsrA mutant was significantly higher than that for the ΔmsrAΔmsrAB double mutant. The highest specific glucose uptake rate (qglucose) was measured for the ΔmsrAΔmsrAB double mutant, indicating that glucose supports higher glycolytic fluxes in the absence of Msr. As with the WT strain, glucose was mainly metabolized into lactate by mutant strains, and no difference in terms of lactate secretion yield was observed (Table 1). However, the ΔmsrA and ΔmsrAΔmsrAB mutants produced more acetate and smaller amounts of succinate than the ΔmsrAB mutant and WT strains. The ΔmsrAΔmsrAB double mutant accumulated higher levels of acetate in the growth medium than the ΔmsrA single mutant. Taken together, these data suggest that MsrA mediates a much more significant regulatory effect on fermentative metabolism than MsrAB, and that, together, the two proteins may contribute to the regulation of carbon flow at the pyruvate node.

3.3. Met(O) Accumulation in msr Mutant Proteomes

Since the lack of Msr activity makes cellular proteome and exoproteome more susceptible to oxidation [27], we compared the total Met(O) peptide content of cellular (Table S1) and extracellular (Table S2) protein samples harvested at EE, LE and S growth phase from cultures of msr mutants and WT strains (Figure 2). The Met(O) peptide content was estimated as a percentage of the total number of peptides identified in each of the three biological replicates obtained from each growth phase. The data showed no significant changes in intracellular Met(O) peptide content as growth progressed for any strain (Figure 3a). However, higher Met(O) levels were detected in ΔmsrA and ΔmsrAΔmsrAB mutant strains compared to ΔmsrAB mutant and WT strains regardless of the growth phase, and in the ΔmsrΔAmsrAB double mutant compared to the msrA single mutant at the EE and LE growth phases. Met(O) peptide content accounted for 8% of all peptides expressed by the ΔmsrAΔmsrAB mutant at the beginning of the exponential growth phase (EE). No significant differences in extracellular Met(O) were found between the mutant and the parental strains (Figure 3b). Met(O) accounted for up to 13% of the total extracellular peptide count. Taken together, these data show that MsrA is a major contributor to the regulation of cellular proteome-wide methionine oxidation under anaerobiosis, whereas MsrAB appears to play a minor role in this process.

3.4. Identification of Putative Msr Substrates

Proteins carrying MetO residues that are differentially oxidized in msr mutants are likely to be substrates for Msr. To identify Msr substrates, we considered that a peptide contained Met(O) residues (Met(O) peptide) when the oxidized form was detected in a least two biological replicates at different time-points. On this basis, we identified 476 Met(O) peptides in cellular extracts (Table S1) and 370 Met(O) peptides in extracellular extracts (Table S2). We then examined changes in Met(O) levels in these peptides. Only peptides for which the Met(O) content changed more than 1.5-fold in at least one mutant strain compared to WT (adjusted p-value < 0.05) were selected. Based on this criterion, 43 Met(O)-peptides from 15 proteins were confidently identified from cellular extracts (Table 2), and 35 Met(O)-peptides from 21 proteins were identified from extracellular extracts (Table 3). To exclude any influence of bias in protein abundance on the observed differences in levels of Met(O), we performed, in parallel, a differential proteomics analysis on the 998 cellular proteins and 433 exoproteins validated by at least two peptides (Tables S3 and S4). The statistical criteria applied were the same as those used to determine the Met(O) level. This analysis revealed 43 cellular proteins (Table S5) and 41 extracellular proteins (Table S6) for which significant abundance changes were detected. Two cellular proteins, the glycolytic enzyme glucose 6-phosphate isomerase and the protein Gls24, were found to be increased both in terms of their Met(O) content (Table 2) and their abundance in ΔmsrA and ΔmsrAΔmsrAB mutants compared to WT (Table S5). Both the Met(O) level and overall abundance of four extracellular proteins were decreased in mutant strains compared to WT (Table 3 and Table S6). Among these proteins, three (flagellins FlaA, FlaB and FlaC) are components of the flagellar apparatus. Finally, out of the 15 proteins listed in Table 2, thirteen are potential substrates of Msr, whereas, out of the 21 extracellular proteins listed in Table 3, seventeen may be potential substrates of Msr.

3.4.1. Putative Msr Substrates Identified in B. cereus Cellular Proteome

According to our criteria, no significant differences in abundance for individual protein-bound Met(O) residues were found between the ΔmsrAB mutant and WT strains, regardless of the growth phase. In contrast, in ΔmsrA and/or ΔmsrAΔmsrAB mutants, a higher Met(O) content was detected for 32 Met residues compared to the levels present in WT (Table 2). The abundance levels for the corresponding 13 proteins were unchanged (Table S5). Interestingly, we noted that the highest number of Met(O) level changes in ΔmsrA and/or ΔmsrAΔmsrAB mutants was detected in samples harvested during the LE growth phase. These results indicate that MsrA has a broader substrate range than MsrAB, and that the impact of MsrAB deficiency was minor in the absence of MsrA.
The translation elongation factor Ef-Tu (Tuf)—one of the most abundant proteins in cells—contains the largest number of MsrA-Met(O) targets, representing 83% of its total Met content. The chaperonin GroEL was also found to contain a high number of Met(O) susceptible to MsrA reduction (five residues), representing 25% of its Met content. The Met content of glycolytic enzymes enolase (Eno) and glyceraldehyde-3-phosphate dehydrogenase (GapA2) was 45% more oxidized in the absence of MsrA. Several other enzymes classed as involved in energy metabolism were found to be more oxidized in ΔmsrA mutant strains. These enzymes included the fermentative enzyme alcohol dehydrogenase (AdhE), the glycolytic enzyme pyruvate kinase (Pyk), the fermentative enzyme lactate dehydrogenase (Ldh2), and the alpha subunit of ATP synthase/hydrolase (AtpA). However, in contrast to Eno and GapA2, each of these enzymes contained only one MsrA-Met(O) target, and their Met(O) residues represented no more than 14% of their total Met content. Regardless of the number of Met(O) targets, many of these proteins corresponded to key enzymes in the energy metabolism.

3.4.2. Putative Msr Substrates Identified in B. cereus Exoproteome

Many of the proteins identified as putative Msr substrates in B. cereus exoproteome were typical exoproteins, including exotoxins and degradative enzymes (Table 3). Changes in their Met(O) content were observed mainly during the LE growth phase in all three mutant strains—ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB—indicating that some of their Met(O) residues can be substrates of both MsrA and MsrAB. Degradative enzymes contained no more than two Met residues for which increasing Met(O) levels were detected. Overall, exotoxins contained more Met(O) residues than other proteins. Specifically, Hbl components contained the highest number of Met(O) residues, with 37.5 and 50% of total Met residues in the lytic component HblL1 and the binding component HblB, respectively. In conclusion, our results indicate that several virulence factors secreted by B. cereus, including toxins and degradative enzymes, are putative Msrsubstrates under anaerobiosis, particularly during the LE growth phase.

3.5. Swimming Motility of B. cereus Depends on MsrA Activity

Our proteomics results indicated that MsrA activity was essential to maintain the abundance level of flagellins (which drive B. cereus motility [42]). We therefore investigated swimming and swarming motility for the WT strain and compared it to that of the ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB mutants under anaerobiosis. Data were evaluated by a Student t-test. No significant difference in cell migration capacity was observed between WT and mutant strains on media supporting swarming. In contrast, as shown in Figure 4, the ΔmsrA and the ΔmsrAΔmsrAB mutants gave rise to significantly smaller colonies (diameter 5.0 ± 0.0 mm) than those produced by the WT and ΔmsrAB mutant strains (diameters 10.7 ± 0.6 and 10.3 ± 0.6 mm, respectively; p-value < 0.01). This reduced diameter suggests that B. cereus swimming motility was significantly reduced in the absence of MsrA.

4. Discussion

The aim of this study was to investigate the antioxidant role of Msr proteins under anaerobic fermentative growth conditions by a proteomics approach. MsrA and MsrAB are two methionine sulfoxide reductases predicted to reverse oxidative damage to methionine in B. cereus. The genes encoding these two Msr are transcribed independently, and our results show that they share similar expression patterns over the course of fermentative anaerobic growth. Thus, expression of msr genes is growth-phase dependent and reached its maximum during the LE growth phase under anaerobiosis; under aerobiosis, this maximum was reached during the stationary phase [27]. This expression profile suggests that Msr are required earlier when cells are grown under anaerobiosis compared to under oxic conditions, perhaps as a means to repair accumulated oxidative damage [43]. The contributions of MsrA and MsrAB to the reduction of cellular Met(O)-bound proteins were clearly distinct under fermentative anaerobic conditions. The extended substrate range of MsrA compared to MsrAB could explain the major role played by MsrA compared to MsrAB in B. cereus fermentative growth.
In contrast to MsrAB, a lack of MsrA significantly changed the oxidation status of Met residues in several cellular proteins including the GroEL chaperone, the elongation factor Ef-Tu, the alpha component of the F1F0-ATPase complex and key enzymes involved in central metabolic processes, which led to concomitant changes in the distribution of metabolic fluxes (Figure 5).
GroEL is a Met-rich chaperone that functions in vivo to fold newly synthetized peptides. The chaperonin activity of GroEL needs ATP [44] and, in Escherichia coli, depends on a Msr-mediated repair system under oxic growth conditions [45]. In Helicobacter pylori, the Msr-mediated repair of GroEL serves to protect catalase against oxidative damage [46]. The elongation factor Ef-Tu is a translational GTPase that plays a central role during the elongation phase of protein synthesis in bacteria and eukaryotes. It also displays diverse moonlighting functions related to bacterial pathogenesis [47]. In eukaryotes, Msr-based repair systems preserve the activity of Ef-Tu and other complexes to maintain protein biogenesis [16,17]. Under fermentative conditions and in the absence of oxidative phosphorylation, the F0F1 ATPase complex hydrolyzes ATP and plays a key role in the H+ transport accompanying certain secondary transporters and/or enzymes involved in anaerobic oxidation–reduction [48]. Impairment of F0F1 as a result of enhanced Met oxidation of one of its components could increase its turnover and ATP requirements, leading to perturbed fermentative metabolism (Table 1). Changes to the oxidation status of glycolytic enzymes and fermentative enzymes, and thus in their activities [49], could also contribute to perturbing fermentative metabolism. The lactate pathway is the main fermentative pathway regenerating NAD+ from NADH in B. cereus [2]. Indeed, during pyruvate oxidation, B. cereus produces significantly more lactate than succinate and ethanol (Table 1). Lactate and ethanol production were unchanged in the absence of MsrA, whereas succinate formation was decreased. However, due to the minor impact of the succinate pathway on NAD+ generation, this decrease probably has a neutral effect on the cellular redox balance. The acetate pathway does not involve redox reactions and generates additional ATP outside of glycolysis through the conversion of acetyl-CoA to acetate (Figure 5). In the absence of MsrA, acetate secretion is increased, indicating a higher carbon flow through acetate pathway, and a concomitantly higher ATP production. To sustain high carbon flow through the acetate pathway, ΔmsrA and ΔmsrAΔmsrAB mutants increase carbon flow through glycolysis, as revealed by increased glucose consumption (Table 1). Finally, when MsrA is lacking, B. cereus adjusts its fermentative metabolism to maintain redox balance and promote ATP synthesis, probably to sustain—for as long as possible—repairing processes that have become less efficient due to the absence of Msr, and F0F1 ATPase complex deficiency.
In terms of capacity to colonize an environment, in the absence of MsrA, B. cereus cells showed reduced motility. This result appears logical as the bacterial flagellum is responsible for motility [50], and synthesis of some flagellar components was observed to be reduced in the absence of MsrA, possibly as a result of an overoxidation of their Met residues [51]. Down-regulation of flagellar components in a context where ATP demand is increased may help cells to maintain growth. The flagellum is a potential virulence factor along the same lines as degradative enzymes and exotoxins. All these virulence factors contain several Met(O), are highly produced at the end of growth [52], and are exported in an unfolded form [53]. Msr are known to preferentially reduce unfolded oxidized proteins [17], suggesting that these virulence factors, especially enterotoxin Hbl, could be repaired by cytoplasmic Msr before their secretion. Whether Msr-dependent Met oxidation regulates exotoxin secretion, structure and activity remains an open question. However, as reported for other pathogens [54], it is probable that Msr contributes to B. cereus virulence under both anaerobiosis and aerobiosis [27].
In contrast to MsrA, a lack of MsrAB had little effect on B. cereus fermentative metabolism. Although it has a minor impact compared to MsrA, the role of MsrAB is, nevertheless, important as it contributes to the intracellular accumulation of Met(O) (Figure 3), and to fermentative metabolism in the absence of MsrA. This observation suggests that MsrA could have a higher affinity than MsrAB for surface-accessible Met(O) within cellular proteins, and that MsrA and MsrAB could cooperate to reduce Met(O) in some proteins. Differences in Met(O) reduction activity between MsrAB and MsrA were less marked when examining extracellular proteins, suggesting that the affinity differences between the two enzymes could be less significant when dealing with unfolded proteins.

5. Conclusions

Even though MsrA and MsrAB seem to be present at very low levels in anaerobic fermentative B. cereus cells, they are part of a highly regulated machinery controlling energy metabolism and, possibly, virulence (Figure 5). In addition, our study indicates that the oxidation of methionine residues in proteins may be an inevitable side effect of life, whether under anaerobic or aerobic conditions.

Supplementary Materials

The following are available online at https://0-www-mdpi-com.brum.beds.ac.uk/article/10.3390/antiox10050819/s1, Figure S1: Analysis of msrA expression under aerobiosis, Table S1: Peptides containing oxidized methionine identified in the cellular proteomes of the B. cereus ΔmsrA, ΔmsrAB, ΔmsrAΔmsrAB and wild-type (WT) strains, Table S2: Peptides containing oxidized methionine identified in the exoproteomes of the B. cereus ΔmsrA, ΔmsrAB, ΔmsrAΔmsrAB and wild-type (WT) strains, Table S3: Proteins identified in the cellular proteome of the B. cereus ΔmsrA, ΔmsrAB, ΔmsrAΔmsrAB and wild-type (WT) strains, Table S4: Proteins identified in the exoproteome of the B. cereus ΔmsrA, ΔmsrAB, ΔmsrAΔmsrAB and wild-type (WT) strains, Table S5: Cellular proteins showing differential accumulation between ΔmsrA, ΔmsrAB or ΔmsrAΔmsrAB with respect to wild-type (WT), Table S6: Extracellular proteins showing differential accumulation between ΔmsrA, ΔmsrAB or ΔmsrAΔmsrAB with respect to wild-type (WT).

Author Contributions

Conceptualization, C.D.; methodology, J.-P.M., M.F., B.A.-B. and C.D.; validation, C.D., B.A.-B. and J.A.; formal analysis, B.A.-B. and C.D.; writing—original draft preparation, C.D.; writing—review and editing, C.D., B.A.-B. and J.A.; All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The data presented in this study are openly available in the PRIDE partner repository under dataset identifiers PXD024888 for the cellular proteome of B. cereus ATCC 14579, PXD024927 for the cellular proteome of the ΔmsrAB mutant, PXD024850 for the cellular proteome of ΔmsrA mutant, PXD024849 for the cellular proteome of ΔmsrABΔmsrA mutant, PXD024702 for the exoproteome of B. cereus ATCC 14579, PXD024714 for the exoproteome of ΔmsrAB mutant, PXD024847 for the exoproteome of ΔmsrA mutant and PXD024848 for the exoproteome of the ΔmsrABΔmsrA mutant.

Acknowledgments

We thank Soria Benhaddi for the very efficient technical help provided.

Conflicts of Interest

The authors declare no conflict of interest.

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Figure 1. Analysis of msrA and msrAB gene expression in B. cereus ATCC 14579 cells grown under anaerobiosis. mRNA levels of msrA (green) and msrAB (blue) were determined at the early exponential (EE), late exponential (LE) and stationary (S) growth phases by quantitative real-time RT-PCR and normalized to ssu mRNA levels. Samples were harvested as indicated in Figure 2. Data correspond to the mean ± SD of six samples (two technical replicates x three biological replicates). Data denoted by a common letter are not significantly different. Data denoted by different letters indicated a significant difference (two-way ANOVA followed by Tukey’s multiple comparison post hoc analysis, p ≤ 0.05).
Figure 1. Analysis of msrA and msrAB gene expression in B. cereus ATCC 14579 cells grown under anaerobiosis. mRNA levels of msrA (green) and msrAB (blue) were determined at the early exponential (EE), late exponential (LE) and stationary (S) growth phases by quantitative real-time RT-PCR and normalized to ssu mRNA levels. Samples were harvested as indicated in Figure 2. Data correspond to the mean ± SD of six samples (two technical replicates x three biological replicates). Data denoted by a common letter are not significantly different. Data denoted by different letters indicated a significant difference (two-way ANOVA followed by Tukey’s multiple comparison post hoc analysis, p ≤ 0.05).
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Figure 2. Growth curves for B. cereus wild-type and msr mutant strains under anaerobic fermentative conditions. Wild-type strain ATCC 14579 (black), ΔmsrA (green), ΔmsrAB (blue), and ΔmsrAΔmsrAB mutants (red) were grown in MOD medium supplemented with 30 mM glucose. Data correspond to the mean ± SD of three biological replicates.
Figure 2. Growth curves for B. cereus wild-type and msr mutant strains under anaerobic fermentative conditions. Wild-type strain ATCC 14579 (black), ΔmsrA (green), ΔmsrAB (blue), and ΔmsrAΔmsrAB mutants (red) were grown in MOD medium supplemented with 30 mM glucose. Data correspond to the mean ± SD of three biological replicates.
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Figure 3. Met(O) content of B. cereus wild-type and msr mutant proteomes under anaerobic fermentative conditions. Wild-type strain ATCC 14579 (black), ΔmsrA (green), ΔmsrAB (blue), and ΔmsrAΔmsrAB mutants (red), were grown in MOD medium supplemented with 30 mM glucose. Samples were collected at early exponential (EE), late exponential (LE), and stationary (S) growth phases, as indicated in Figure 2. The relative Met(O) content in the cellular proteome (a) and exoproteome (b) was calculated as a percentage of oxidized methionine-containing peptides with respect to the total number of methionine-containing peptides identified in samples for each growth phase. Data correspond to the mean ± SD of three biological replicates. Within each panel, data denoted by a common letter are not significantly different. Data designed by different letters indicated a significant difference (two-way ANOVA followed by Tukey’s multiple comparison post hoc analysis, p ≤ 0.05).
Figure 3. Met(O) content of B. cereus wild-type and msr mutant proteomes under anaerobic fermentative conditions. Wild-type strain ATCC 14579 (black), ΔmsrA (green), ΔmsrAB (blue), and ΔmsrAΔmsrAB mutants (red), were grown in MOD medium supplemented with 30 mM glucose. Samples were collected at early exponential (EE), late exponential (LE), and stationary (S) growth phases, as indicated in Figure 2. The relative Met(O) content in the cellular proteome (a) and exoproteome (b) was calculated as a percentage of oxidized methionine-containing peptides with respect to the total number of methionine-containing peptides identified in samples for each growth phase. Data correspond to the mean ± SD of three biological replicates. Within each panel, data denoted by a common letter are not significantly different. Data designed by different letters indicated a significant difference (two-way ANOVA followed by Tukey’s multiple comparison post hoc analysis, p ≤ 0.05).
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Figure 4. Swimming motility. Representative colonies of wild-type (WT) and ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB mutants following growth on swimming TrA plates for 72 h under anaerobiosis.
Figure 4. Swimming motility. Representative colonies of wild-type (WT) and ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB mutants following growth on swimming TrA plates for 72 h under anaerobiosis.
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Figure 5. Schematic view of the roles of MsrA and MsrAB on B. cereus physiology under anaerobic fermentative conditions. MsrA has a more important role in fermentative metabolism, compared to MsrAB (thick green vs. thin blue solid arrows). The role of MsrA could be as important as the role of MsrAB in maintaining Met(O) levels of virulence factors, such as flagella and enterotoxins (green and blue dotted arrows). PTS, phosphotransferase system; PP, pentose phosphate pathway. Succinate is formed via the reductive TCA cycle.
Figure 5. Schematic view of the roles of MsrA and MsrAB on B. cereus physiology under anaerobic fermentative conditions. MsrA has a more important role in fermentative metabolism, compared to MsrAB (thick green vs. thin blue solid arrows). The role of MsrA could be as important as the role of MsrAB in maintaining Met(O) levels of virulence factors, such as flagella and enterotoxins (green and blue dotted arrows). PTS, phosphotransferase system; PP, pentose phosphate pathway. Succinate is formed via the reductive TCA cycle.
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Table
Table 1. Growth parameters and end product yields obtained for anaerobic batch cultures of ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB mutants, and their parental strain, B. cereus ATCC 14579 (WT).
Table 1. Growth parameters and end product yields obtained for anaerobic batch cultures of ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB mutants, and their parental strain, B. cereus ATCC 14579 (WT).
B. cereus Strains
WTΔmsrAΔmsrABΔmsrAΔmsrAB
µmax (h−1)1.0 ± 0.1 a1.0 ± 0.1 a0.9 ± 0.1 a1.0 ± 0.1 a
Final OD6002.0 ± 0.1 a1.4 ± 0.2 b2.0 ± 0.1 a1.1 ± 0.1 c
Final biomass (g/L)0.8 ± 0.1 a0.6 ± 0.1 b0.8 ± 0.1 a0.4 ± 0.1 c
qglucose (mmol/g/h)77 ± 7 a96 ± 4 b103 ± 5 b168 ± 5 c
Yacetate (mol/mol)0.31 ± 0.01 a0.41 ± 0.01 b0.24 ± 0.01 c0.65 ± 0.04 d
Ylactate (mol/mol)1.45 ± 0.06 a1.52 ± 0.01 a1.57 ± 0.06 a1.47 ± 0.42 a
Yformate (mol/mol)0.39 ± 0.08 a0.47 ± 0.01 a0.31 ± 0.08 a0.44 ± 0.07 a
Yethanol (mol/mol)0.10 ± 0.00 a0.07 ± 0.02 a0.10 ± 0.00 a0.08 ± 0.02 a
Ysuccinate (mol/mol)0.04 ± 0.00 a0.00 ± 0.00 b0.05 ± 0.00 a0.00 ± 0.00 b
abc Within a row, means ± SD without a common superscript significantly differ (Student’s t test, p ≤ 0.05).
Table
Table 2. Cellular peptides for which significant fold-changes in Met(O) levels (ǀlog2 FCǀ ≥ 1.5, adjusted p value ≤ 0.05) were detected in cellular extracts from ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB compared to WT at early exponential growth phase (EE), late exponential growth phase (LE) and stationary growth phase (S).
Table 2. Cellular peptides for which significant fold-changes in Met(O) levels (ǀlog2 FCǀ ≥ 1.5, adjusted p value ≤ 0.05) were detected in cellular extracts from ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB compared to WT at early exponential growth phase (EE), late exponential growth phase (LE) and stationary growth phase (S).
Molecular FunctionGene NoProtein NameDescriptionMet(O)/
Total Met		Met(O) Peptide Detected by LC MS/MS alog2FC b
EELES
ΔmsrAΔmsrAΔmsrABΔmsrAΔmsrAΔmsrABΔmsrAΔmsrAΔmsrAB
Amino acid metabolismBC1238TrpATryptophan synthase, alpha subunit1/5EVQMPFVLMTYLNPVLAFGK 4.2
ATP synthesisBC5308AtpAF0F1 ATP synthase, alpha subunit1/10IMQVPVGK 2.3
Chaperone proteinsBC0295GroELChaperonin 5/20SALQNAASVAAMFLTTEAVVADKPEPNAPAMPDMGGMGMGGMGGMM 3.3
NVTAGANPMGLR 2.0−3.0
SSIAQVAAISAADEEVGQLIAEAMER3.0 3.94.54.0
AMLEDIAILTGGEVITEELGR4.55.04.34.64.74.3
Degradative enzymesBC1991TgCPutative murein endopeptidase1/9YKQSMDGTMQDIKK −3.3
FermentationBC4365AdhEbifunctional acetaldehyde-CoA alcohol dehydrogenase4/30QLMNHDGVALVLATGGAGMVK 3.2
MIDTLVNNGQQALQALESFTQEEIDNIVHEMALAGVDQHMPLAK 2.63.0
LPLISELKEIYMK2.8 3.24.3
BC4870Ldh2L-lactate dehydrogenase1/7GIMDSGFDGIFLIATNPVDILTYVTWK 3.2 4.83.7
GlycolysisGluconeogenesisBC4599PykIPyruvate kinase1/16AASTDEMLDTAIQTGMDAGLIGLGDTVVITAGVPVAETGTTNLMK2.7 3.44.03.83.4
BC4898 cPgiGlucose-6-phosphate isomerase2/9FSVLTPVGLLPIAVSGLNIEEMMK 3.1
FSVLTPVGLLPIAVSGLNIEEMMK2.93.53.94.84.34.4
BC5135EnoPhosphopyruvate hydratase5/11QLPTPMMNIINGGSHADNNVDFQEFMILPVGAPTFK 2.6
VNQIGTLTETFEAIEMAKR3.1 3.0
QLPTPMMNIINGGSHADNNVDFQEFMILPVGAPTFK2.53.43.33.9
AMIELDGTPNKGK−2.6 −2.6 -2.4
LGANAILGVSMAVAHAAADFVGLPLYR3.53.73.33.6 2.9
AMIELDGTPNK −2.9
BC5140GapA2Glyceraldehyde-3-phosphate dehydrogenase4/9GMMTTIHSYTNDQQILDLPHK 3.8
GILGYSEEPLVSIDYNGCTASSTIDALSTMVMEGNMVK 3.0
GMMTTIHSYTNDQQILDLPHKDLR 3.0
GILGYSEEPLVSIDYNGCTASSTIDALSTMVMEGNMVK3.0 4.14.0
AAAENMIPTSTGAAK−2.3 −2.3
Protein exportBC4410YajCPreprotein translocase 1/6AVAQMQSELAK−3.2
Translation apparatusBC0129TufElongation factor Tu10/12CDMVDDEELLELVEMEVR 3.9
CDMVDDEELLELVEMEVRDLLSEYGFPGDDIPVIK 3.9
ETDKPFLMPVEDVFSITGR 2.8 4.33.1
IIELMAEVDAYIPTPERETDKPFLMPVEDVFSITGR 4.64.8
IIELMAEVDAYIPTPERETDKPFLMPVEDVFSITGR4.24.24.45.1
NMITGAAQMDGGILVVSAADGPMPQTR3.43.9
QVGVPYIVVFLNKCDMVDDEELLELVEMEVR 3.5
TTDVTGIIQLPEGTEMVMPGDNIEMTIELIAPIAIEEGTK3.1 3.63.94.54.3
TTDVTGIIQLPEGTEMVMPGDNIEMTIELIAPIAIEEGTK3.1 3.13.43.93.4
TTDVTGIIQLPEGTEMVMPGDNIEMTIELIAPIAIEEGTK 4.04.33.73.6
TTDVTGIIQLPEGTEMVMPGDNIEMTIELIAPIAIEEGTK 3.23.3
TTDVTGIIQLPEGTEMVMPGDNIEMTIELIAPIAIEEGTK 2.9
VGDVVEIIGLAEENASTTVTGVEMFR 5.14.0
VGDVVEIIGLAEENASTTVTGVEMFRK 6.16.14.4
BC5471RplI50S ribosomal protein L91/4QGLAAEATNSSMK −5.0−4.6−4.7−5.6
BC0155Rpm50S ribosomal protein L361/2VMVICENPK −2.9
UncategorizedBC4182 cGls24Unknown1/6VEIAPEVIEVIAGIAAAEVEGVAAMR2.7 3.2 3.93.2
a Met(O) residues that showed significant level changes are indicated in bold. b Only significant log2FC changes are reported. c Shaded lines show cellular proteins for which significant abundance changes were detected: the two highlighted proteins showed increased abundance in the msr mutant (Table S5).
Table
Table 3. Extracellular peptides for which significant fold-changes in Met(O) level (ǀlog2 FCǀ ≥ 1.5, adjusted p value ≤ 0.05) were detected in samples from cultures of ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB compared to WT at early exponential growth phase (EE), late exponential growth phase (LE) and stationary growth phase (S).
Table 3. Extracellular peptides for which significant fold-changes in Met(O) level (ǀlog2 FCǀ ≥ 1.5, adjusted p value ≤ 0.05) were detected in samples from cultures of ΔmsrA, ΔmsrAB and ΔmsrAΔmsrAB compared to WT at early exponential growth phase (EE), late exponential growth phase (LE) and stationary growth phase (S).
Molecular FunctionGene NoProtein
Name		DescriptionMet(O)/
Total Met		Met(O) Peptide Detected by LC MS/MSalog2FCb
EELES
ΔmsrAΔmsrABΔmsrAΔmsrABΔmsrAΔmsrABΔmsrAΔmsrABΔmsrAΔmsrABΔmsrAΔmsrAB
Cell surface biogenesisBC5196CwlDN-acetylmuramoylL-alanine amidase 3/8MDTVVTSMTSTEGQLKELEK−1.1−1.1−1.0
ILESDEDIMK−0.4−1.5−0.7
ChaperoneBC0295GroELChaperonin 1/20AMLEDIAILTGGEVITEELGR0.81.50.2
Degradative enzymesBC0556ColGCollagenase 1/6GLEVVTQAMHMYPR1.11.11.3
MKGQAIYDIMQGIDYDIQSYLTEAR0.00.00.09.41.29.9
BC0670PlcBPhospholipase C 1/6AEVTPMTGKR2.3−0.12.49.52.610.0
BC1193PepF1Oligoendopeptidase F 1/11ALGLDELHMYDLYTPLVPEVK 23.015.018.9
BC1991TgCMurein endopeptidase 1/9NIMDQLYGEFNKIVDADEYVK 9.4−0.48.7
NIMDQLYGEFNKIVDADEYVKYNVASTR−1.0−0.9−1.0
BC2735NprP2Bacillolysin 2/10GIGEDKMFDIFYYANTDELNMTSNFK 6.51.06.6
GIGEDKMFDIFYYANTDELNMTSNFK 7.51.77.5
BC5351NprBBacillolysin 1/6NMSDIYDYFKK−1.5−1.2−0.4
GNGIYIYNANYADSLGGYSQAGYPGTLISSSTPNFADKEAAGAMK2.50.32.67.71.58.2
FlagellaBC1657 cFlaAFlagellin 2/15ILNEAGISMLSQANQTPQMVSK−3.10.0−3.1
VQLSDASGDTMTIDSLNAK −6.00.1−8.9
BC1658 cFlaBFlagellin 1/15TNFNGNSFLDTTATPPGKDIEIQLSDASGDTMTLK−1.7−0.7−2.4
BC1659 cFlaCFlagellin 1/15LDHNLNNVTSQATNMAAAASQIEDADMAKEMSEMTK−2.6−0.9−2.8
Glycolysis
Gluconeogenesis		BC4898PgiGlucose-6-phosphate isomerase 1/9FSVLTPVGLLPIAVSGLNIEEMMK 7.23.37.2
BC5135EnoPhosphopyruvate hydratase 2/11LGANAILGVSMAVAHAAADFVGLPLYR 9.52.29.6
VNQIGTLTETFEAIEMAK1.81.61.4
ExotoxinsBC3101HblB’Hemolysin BL, component B’ 2/15GLDMVKIPFIPTLIAGGIMIGDAR1.50.9
IPFIPTLIAGGIMIGDAR 7.90.77.9
BC3102HblBHemolysin BL, component B4/8SMNAYSYMLIKNPDVNFEGITINGYVDLPGR 6.30.76.7
MKETLQK0.3−1.00.4
QLLDTLNGIVEYDTTFDNYYETMVEAINTGDGETLKEGITDLR 8.42.27.7
QLLDTLNGIVEYDTTFDNYYETMVEAINTGDGETLK 7.90.97.4
BC3103HblL1Hemolysin BL, component L13/8MLQDFKGK 8.23.78.2
IGELSMKADR1.7−0.32.1
QWNTMGANYTDLLDNIDSMEDHKFSLIPDDLK1.90.81.68.01.57.4
BC3523HlyIIHemolysin II 1/7DSFNTFYGNQLFMK 0.9−5.40.9
BC1809NheANon hemolytic enterotoxin, A1/9VLNNNMIQIQTNVEEGTYTDSSLLQK 7.6−0.38.2
BC5101HlyICereolysin2/7MTLDHYGAYVAQFDVSWDEFTFDQK0.81.00.4
KVMVAAYK 6.3 6.3
Toxin-likeBC5239EntAEnterotoxin, cell wall binding1/5VLTAMGHDLTANPNMK−1.4−1.4−0.6
UncategorizedBC5027 c ErfK/srfK precursor 1/4MYNNDIHWLFER−1.6−0.9−1.0
a Met(O) residues that showed significant level changes are indicated in bold. b Only significant log2FC changes are reported. c Shaded lines show exoproteins for which significant abundance changes were detected: the four highlighted proteins showed decreased abundance in the msr mutant (Table S6).
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Duport, C.; Madeira, J.-P.; Farjad, M.; Alpha-Bazin, B.; Armengaud, J. Methionine Sulfoxide Reductases Contribute to Anaerobic Fermentative Metabolism in Bacillus cereus. Antioxidants 2021, 10, 819. https://0-doi-org.brum.beds.ac.uk/10.3390/antiox10050819

AMA Style

Duport C, Madeira J-P, Farjad M, Alpha-Bazin B, Armengaud J. Methionine Sulfoxide Reductases Contribute to Anaerobic Fermentative Metabolism in Bacillus cereus. Antioxidants. 2021; 10(5):819. https://0-doi-org.brum.beds.ac.uk/10.3390/antiox10050819

Chicago/Turabian Style

Duport, Catherine, Jean-Paul Madeira, Mahsa Farjad, Béatrice Alpha-Bazin, and Jean Armengaud. 2021. "Methionine Sulfoxide Reductases Contribute to Anaerobic Fermentative Metabolism in Bacillus cereus" Antioxidants 10, no. 5: 819. https://0-doi-org.brum.beds.ac.uk/10.3390/antiox10050819

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