|A RubisCO-like protein links SAM metabolism with isoprenoid biosynthesis.|
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|PMID: 23042035 Owner: NLM Status: MEDLINE|
|Functional assignment of uncharacterized proteins is a challenge in the era of large-scale genome sequencing. Here, we combine in extracto NMR, proteomics and transcriptomics with a newly developed (knock-out) metabolomics platform to determine a potential physiological role for a ribulose-1,5-bisphosphate carboxylase/oxygenase (RubisCO)-like protein from Rhodospirillum rubrum. Our studies unraveled an unexpected link in bacterial central carbon metabolism between S-adenosylmethionine-dependent polyamine metabolism and isoprenoid biosynthesis and also provide an alternative approach to assign enzyme function at the organismic level.|
|Tobias J Erb; Bradley S Evans; Kyuil Cho; Benjamin P Warlick; Jaya Sriram; B McKay Wood; Heidi J Imker; Jonathan V Sweedler; F Robert Tabita; John A Gerlt|
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|Type: Journal Article; Research Support, N.I.H., Extramural; Research Support, Non-U.S. Gov't Date: 2012-10-07|
|Title: Nature chemical biology Volume: 8 ISSN: 1552-4469 ISO Abbreviation: Nat. Chem. Biol. Publication Date: 2012 Nov|
|Created Date: 2012-10-18 Completed Date: 2013-02-12 Revised Date: 2013-07-11|
Medline Journal Info:
|Nlm Unique ID: 101231976 Medline TA: Nat Chem Biol Country: United States|
|Languages: eng Pagination: 926-32 Citation Subset: IM|
|Institute for Genomic Biology, University of Illinois at Urbana-Champaign, Champaign, IL, USA.|
|APA/MLA Format Download EndNote Download BibTex|
Magnetic Resonance Spectroscopy
Polyamines / chemistry, metabolism
Rhodospirillum rubrum / enzymology*
Ribulose-Bisphosphate Carboxylase / chemistry, genetics, metabolism*
S-Adenosylmethionine / chemistry, metabolism*
Terpenes / chemistry, metabolism*
Thionucleosides / chemistry, metabolism
Transcriptome / genetics
|P01 GM071790/GM/NIGMS NIH HHS; P01GM071790/GM/NIGMS NIH HHS; R01 GM065155/GM/NIGMS NIH HHS; R01 GM095742/GM/NIGMS NIH HHS; R01GM065155/GM/NIGMS NIH HHS; R01GM095742/GM/NIGMS NIH HHS; U54 GM093342/GM/NIGMS NIH HHS; U54GM093342/GM/NIGMS NIH HHS|
|0/Deoxyadenosines; 0/Polyamines; 0/Terpenes; 0/Thionucleosides; 29908-03-0/S-Adenosylmethionine; 634Z2VK3UQ/5'-methylthioadenosine; EC 188.8.131.52/Ribulose-Bisphosphate Carboxylase|
Journal ID (nlm-journal-id): 101231976
Journal ID (pubmed-jr-id): 32624
Journal ID (nlm-ta): Nat Chem Biol
Journal ID (iso-abbrev): Nat. Chem. Biol.
nihms-submitted publication date: Day: 10 Month: 9 Year: 2012
Electronic publication date: Day: 07 Month: 10 Year: 2012
Print publication date: Month: 11 Year: 2012
pmc-release publication date: Day: 01 Month: 5 Year: 2013
Volume: 8 Issue: 11
First Page: 926 Last Page: 932
PubMed Id: 23042035
|A RubisCO like protein links SAM metabolism with isoprenoid biosynthesis|
|Tobias J. Erb12*§|
|Bradley S. Evans13*|
|Benjamin P. Warlick12|
|B. McKay Wood1|
|Heidi J. Imker1|
|Jonathan V. Sweedler13|
|F. Robert Tabita4|
|John A. Gerlt123|
1Institute for Genomic Biology, University of Illinois at Urbana-Champaign
2Department of Biochemistry, University of Illinois at Urbana-Champaign
3Department of Chemistry, University of Illinois at Urbana-Champaign
4Department of Microbiology, The Ohio State University
|*These authors contributed equally to this work.
§Current address Institute for Microbiology, ETH Zurich, Switzerland.
D-Ribulose-1,5-bisphosphate carboxylase/oxygenase (RubisCO) is the most abundant protein in the biosphere and catalyzes the key reaction in the Calvin-Benson-Bassham cycle, the major process of atmospheric CO2 fixation on earth1,2. To date, three different types of RubisCO are distinguished that all serve as true carboxylases in plants, bacteria, and archaea, respectively. However, recent sequencing projects identified RubisCO homologs (RubisCO-like proteins, RLPs) in a number of bacterial and archaeal genomes, such as Chlorobaculum tepidum, Bacillus subtilis, Pseudomonas putida, Mesorhizobium loti, Archaeoglobus fulgidus, and Rhodospirillum rubrum2. In contrast to true RubisCOs, RLPs lack essential, conserved active site residues. Consequently, none of these proteins tested so far has been shown to catalyze the carboxylation of D-ribulose-1,5-bisphosphate.
Given the importance of RubisCO in the global carbon cycle, much effort has been undertaken to understand the evolutionary relationship and functional diversity within the RubisCO-superfamily and its RLP members3–5. Based on phylogenetic analysis, active site differences and genome context, at least six different RLP-subfamilies were identified that are assumed to use different substrates and catalyze different reactions (Fig. 1a)2. However, correct functional assignments of RLPs are hampered by the fact that i) RubisCO itself is already an inefficient, naturally promiscuous enzyme6–8, and ii) potential substrate libraries of phosphorylated metabolites are not easily accessible. Although initial studies on the Chlorobium tepidum RLP-subfamily had established that RLPs might be involved in some aspect of sulfur metabolism3, the only group of RLPs for which an exact physiological function has been determined is the Bacillus subtilis RLP-subfamily4,9,10. RLPs in this group catalyze an enolization reaction in a bacterial variation of the ubiquitous “methionine salvage pathway” that converts 5′-methylthio-adenosine (MTA), a dead-end product of SAM-dependent polyamine biosynthesis, into L-methionine 4,11,12 (Fig. 1b).
Earlier experiments on the R. rubrum RLP indicated that this enzyme also functions in MTA metabolism. Wild type R. rubrum can grow with MTA as sole source of sulfur; however, disruption of the RLP gene results in a MTA-deficient growth phenotype under aerobic conditions13. Moreover, when incubated in vitro with 5-methylthio-D-ribulose-1-phosphate (MTRu-1P), an intermediate of the canonical methionine salvage pathway, recombinant R. rubrum RLP was shown to catalyze an unprecedented 1,3-isomerization reaction (presumably two successive 1,2-isomerization reactions) to yield a 1:3 mixture of 1-methylthio-ribulose-5-phosphate (MTRu-5P) and 1-methylthio-xylulose-5-phosphate (MTXu-5P) 5. However, despite these apparent links to MTA metabolism, we noticed that the R. rubrum genome lacks most of the canonical methionine salvage pathway genes and, therefore, might use an alternative strategy to utilize MTA aerobically as its sole sulfur source. In addition, the physiological context of the non-stereospecific isomerization reaction observed with recombinant RLP in vitro remained enigmatic to us.
In this study, we combined in extracto-NMR, transcriptomics, proteomics, classical biochemical methods and genetic knock-outs together with a newly developed metabolomics platform to elucidate MTA metabolism in R. rubrum. Our results give evidence for a so far unknown central metabolic pathway, involving R. rubrum RLP, in which the polyamine biosynthesis dead-end product MTA is channelled into isoprenoid metabolism with concomitant release of the volatile gas methanethiol. The proposed MTA-isoprenoid pathway fits to the organism’s physiology and phylogenetic analysis indicate that a number of organisms make use of this metabolic shunt.
In order to elucidate the unknown MTA metabolic pathway in R. rubrum, we first used 1H-NMR to trace the fate of MTA in R. rubrum cell extracts (in extracto-NMR). For that purpose, extracts of R. rubrum were prepared from cells actively growing with MTA as sole sulfur source (generation time td=16.7 ± 3.0 h). Then, these extracts were exchanged into buffered D2O, MTA was added and 1H-NMR spectra were continuously recorded over time (Supplementary Results, Supplementary Fig. 1). MTA was first converted into 5-methylthio-D-ribose-1-phosphate (MTR-1P) with the release of adenine. Subsequently, MTR-1P was isomerized into MTRu-1P (Fig. 2). The overall rate for this reaction sequence (0.7 + 0.3 nmol min−1 mg−1 protein) closely matched the theoretically expected minimal activity for MTA metabolic enzymes (0.6 nmol min−1 mg−1) to sustain the observed growth of R. rubrum, as calculated from the specific aerobic growth rate of R. rubrum on MTA (μ=0.042 + 0.008h−1, Supplementary Fig. 1). Notably, we could demonstrate MTRu-1P formation at comparable rates also in extracts of sulfate-grown cells, suggesting that MTA metabolism serves a housekeeping function in R. rubrum, analogous to the reactions of the classical methionine salvage pathway in B. subtilis14–16. However, in neither extract could metabolites downstream of MTRu-1P be detected by 1H-NMR, indicating that further investigations are limited by the in extracto NMR-method used.
To identify subsequent reactions steps in MTA metabolism by R. rubrum we developed a liquid-chromatography Fourier transform mass spectrometry (LC-FTMS)-based metabolomics platform that would allow a comprehensive analysis of the R. rubrum metabolome upon perturbation with MTA. This platform combines high-resolution mass spectrometry with new semi-automated data analysis tools for the customized, convenient and highly confident assignment of metabolites based on molecular formula determination (see Methods). To find metabolites specifically affected by MTA-perturbation, suspensions of R. rubrum cells actively growing on minimal medium with sulfate as sole sulfur source were shortly deprived in sulfur-free medium (10 min), before they were transferred onto minimal medium with or without MTA as sole sulfur source and incubated for 10, and 20 min, respectively. Then, metabolites were extracted from whole cells and analyzed by the LC-FTMS platform, as shown in Supplementary Figure 2. Of the 1,406 individual peaks observed from extracts of wild type R. rubrum, we identified a total of 25 metabolites (1.8%) that were significantly up-regulated in MTA-fed cells (Supplementary Table 1). In agreement with the in extracto-NMR results, three of the peaks unique to MTA-feeding could be assigned to MTA, MTR-1P, and MTRu-1P, respectively, and were experimentally confirmed by spiking cell extracts with authentic standards (Supplementary Fig. 3). An additional peak (hypoxanthine) could be assigned as an intermediate in bacterial purine metabolism, which is well in line with downstream metabolism of adenine following its release from MTA upon MTR-1P formation. However, much to our surprise three peaks were significantly up-regulated upon feeding of MTA that could be assigned as metabolites of isoprenoid biosynthesis: 1-deoxyxylulose-5-phosphate (DXP), 4-(cytidine-5′-diphospho)-2-C-methyl-D-erythritol (CDP-ME), and 2-C-methyl-D-erythritol-2,4-cyclodiphosphate (c-MEPP). Spiking of cell extracts with standards confirmed these assignments, indicating an unexpected intertwining of MTA metabolism and isoprenoid biosynthesis in R. rubrum (Supplementary Fig. 2). Realizing structural similarities between MTRu-1P and DXP, we hypothesized that DXP is a downstream metabolite of MTA, which is formed by release of the volatile methanethiol (CH3SH) from an intermediate in the pathway. Indeed, DXP formation in R. rubrum increased in a time dependent manner following MTA-feeding (Fig. 3a) as did the release of methanethiol in supernatants of R. rubrum cell suspensions (quantified with 5,5′-dithiobis(-2-nitrobenzoic acid, DTNB17, Fig. 3b). The rate of methanethiol release from MTA-fed cells (4 nmol min−1 OD578−1) was independent of the sulfur source used to grow R. rubrum (Supplementary Fig. 4), again indicating that MTA metabolism is a housekeeping function in this organism. Finally, when testing a RLP disruption strain13, we could neither observe an increase in DXP formation nor in methanethiol release, which confirmed the functional link between MTA metabolism and isoprenoid biosynthesis (Fig. 3c, 3d).
Next, we sought to identify genes important in MTA metabolism. By screening 10,200 transposon mutants of R. rubrum we identified four mutants in three genes that had lost the ability to release methanethiol upon MTA feeding (Supplementary Fig. 5), one of which was a mutant of the RLP gene (rru_A1998). The other two genes encode a putative MTA-phosphorylase (rru_A0361) and a putative MTR-1P isomerase (rru_A0360). Homologs of the three genes are conserved across the genomes of many bacterial species, where they are often organized as two distinct clusters (Supplementary Table 2). One cluster typically consists of the putative MTA-phosphorylase and the putative MTR-1P isomerase, whereas the second cluster comprises the RLP that is in many cases adjacent to a conserved gene encoding a small metal binding protein (cupin). Based on this observation, we consequently also created a cupin disruption strain. None of the mutant strains released methanethiol and consequently also did not show an increase in DXP-formation after MTA feeding, as demonstrated by LC-FTMS metabolomics (Fig. 3c, 3d). LC-FTMS metabolomic analysis enabled an even more detailed picture of each mutant that allowed functional assignments of the corresponding enzymes. The rru_A0361-mutant did not form MTR-1P or any other downstream metabolite, confirming its role as putative MTA-phosphorylase. MTA-metabolism in the rru_A0360-mutant stopped at the level of MTR-1P, according to its proposed role as MTR-1P-isomerase13. The rru_A1998 (rlp)-mutant accumulated MTRu-1P, as expected from the function of the RLP as an MTRu-1P isomerizing enzyme5. Finally, the cupin-mutant accumulated a mixture of MTRu-5P and MTXu-5P, affirming the role of RLP as MTRu-1P isomerase, and the cupin as being involved in processing these molecules (Fig. 3c, Supplementary Fig. 6). Based on these data, we propose the existence of a new bacterial pathway, the MTA-isoprenoid shunt that links SAM-dependent polyamine metabolism and isoprenoid biosynthesis, as summarized in Fig. 4. In this pathway, MTA, which is derived from polyamine biosynthesis, is first transformed into MTR-1P. MTR-1P is further isomerized to MTRu-1P, which then serves as substrate for the RLP. Due to the combined action of the RLP and the cupin protein, methanethiol is released, the phosphorylated ketose-coproduct is converted into DXP and further channeled into isoprenoid biosynthesis. Note that this proposed reaction sequence is also well supported by MTA-feeding metabolomics of R. rubrum wild type that showed the increase of all major metabolites of the proposed MTA-isoprenoid shunt over time, compared to (non-fed) control cells (Fig. 4).
Although our MTA-feeding (knock-out) metabolomics approach established the functional link between methanethiol release and DXP formation, and consequently the existence of the MTA-isoprenoid shunt, we still worried about the physiological relevance of this pathway in vivo in the absence of exogenous added MTA. For that purpose the metabolomes of R. rubrum wild type cells and mutants that had been grown on minimal medium with sulfate as sole sulfur source were analyzed for metabolites of the proposed MTA-isoprenoid shunt. Wild type R. rubrum contained some MTA-derived metabolites (i.e., MTR-1P), but only at a very low level. This is expected12, as metabolic flux through this pathway is small, because sulfur makes only up to 1.5% of the cellular dry mass18, and spermidine is synthesized at low rates19. In contrast, levels of MTA-derived metabolites were approximately 50 times higher in R. rubrum mutants than in wild type, indicating accumulation of metabolites in the mutants, with individual patterns resembling those of the MTA-feeding experiments (Fig. 5). Notably, when grown with sulfate as sole sulfur source, the mutant strains appeared slightly less colored than wild type R. rubrum and had a lowered carotenoid content (Supplementary Fig. 7), indicating that isoprenoid biosynthesis is indeed fueled to some extent from MTA in vivo. In summary our results suggested that the proposed MTA-isoprenoid shunt is active in vivo and does not require addition of external MTA.
To confirm the biochemistry of the MTA-isoprenoid shunt, we expressed the proteins of the proposed pathway heterologously (Supplementary Fig. 8) and tested their activity in vitro. Rru_A0360 and Rru_A0361 were successfully confirmed as bona fide MTA-phosphorylase and MTR-1P-isomerase, respectively (Supplementary Table 3), whereas the RLP reaction had been demonstrated previously5. Initial experiments to reconstitute the complete methanethiol-releasing reaction sequence in vitro failed. Any efforts to monitor methanethiol release by 1H-NMR with purified proteins (Rru_A0360, RruA_0361, RLP and cupin) from MTA, or MTR-1P were unsuccessful, as were experiments in which methanethiol formation was assayed with O-acetylL-homoserine sulfhydrylase (see below). Similarly, when we incubated purified cupin with the products of the RLP reaction (MTXu-5P/MTRu-5P) we could neither observe methanethiol release nor DXP formation by 1H-NMR or mass spectrometry, indicating that an essential factor might be missing in these experiments. However, when we provided DTT to the reaction mixture, purified cupin was able to release methanethiol preferably from MTXu-5P yielding DXP, as shown by 1H-NMR and LC-FTMS (Supplementary Fig. 9 and 10). This reaction was dependent on both the presence of cupin and stoichiometric amounts of DTT to go to completion, suggesting an unprecedented reductive release of the methanethiol group, that differs from other thiol releasing reactions described so far (e.g., the elimination of homocysteine from S-ribosylhomocysteine in the biosynthesis of the quorum sensing-molecule AI-220).
In summary, our results demonstrated the functionality of the proposed MTA-isoprenoid shunt with purified enzymes in vitro. Yet, we wondered about the relevance of this reaction sequence in vivo, i.e., in the absence of external added reducing equivalents. We therefore developed an assay to monitor the release of methanethiol from MTR-1P, in which extracts of wild type or mutant R. rubrum cells were incubated with MTR-1P (or MTA) and the volatile methanethiol was trapped with a DTNB-soaked filter paper. For wild type extracts, release of methanethiol from MTR-1P was quantified as 0.3 μM min−1 mg−1, whereas methanethiol releasing activity was negligible in mutant cell extracts. However, methanethiol release in extracts of individual mutants could be successfully restored by addition of the respective missing enzyme. These experiments established the role of each protein in methanethiol release, eliminated the possibility of polar effects from mutagenesis, and confirmed the presence of an appropriate reducing equivalent in vivo (Supplementary Fig. 11).
Finally, to identify reactions and enzymes following the release of methanethiol, we compared the proteomes of MTA- and sulfate-grown cells. Five proteins were identified that were highly up-regulated during growth on MTA as sole sulfur source (Supplementary Table 4); among these were two putative O-acetyl-homoserine sulfhydrylases (Rru_A0774, Rru_A0784). Notably, four of these five proteins (Rru_A0779, Rru_A0792, and the two sulfhydrylases) were encoded by the same genetic region of fourteen different genes presumably involved in thiol metabolism at the level of cysteine and methionine (“thiol cluster”, Fig. 6). A complementary transcriptome analysis using mRNA sequencing confirmed the results of the proteomic study and allowed a more detailed view on the differences between MTA- and sulfate-grown cells. Whereas the relative transcript levels of the majority (>99%) of the 3933 annotated genes of R. rubrum remained essentially unchanged for both conditions, including the genes involved in methanethiol release in agreement with their housekeeping function, the relative levels of transcripts for all fourteen genes of the “thiol cluster” were increased between 30- and 320-fold in MTA-grown cells (Supplementary Table 5, Fig. 6). Although this expression pattern resembled a generalized stress response by sulfur deprivation, we realized that expression of the “thiol cluster” and its putative O-acetyl-L-homoserine sulfhydrylases would provide R. rubrum with the metabolic capability to recapture methanethiol in the form of methionine, as reported recently21,22. Indeed, biochemical characterization of heterologously expressed Rru_A0774 confirmed the enzyme as methanethiol-specific O-acetyl-L-homoserine sulfhydrylase (Supplementary Table 3). This closed the gap between methanethiol release and methionine formation, explaining how R. rubrum recycles methanethiol when grown with MTA as sole sulfur source (Fig. 4).
In conclusion, our results give evidence for the existence of two so far unknown pathways in bacterial central metabolism: first, methanethiol release from MTA represents an alternative strategy to metabolize the dead-end product MTA besides the classical methionine salvage pathway4,11,12. At the same time, conversion of the remaining portion of MTRu-1P into DXP represents a new biosynthetic route to this isoprenoid precursor as an alternative to the well characterized non-mevalonate23,24 pathway that prevails in many bacteria. Although R. rubrum encodes DXP synthase (Rru_A1592), the key enzyme of the non-mevalonate pathway that might provide most of the DXP in R. rubrum, the MTA-isoprenoid shunt, as proposed here, could also contribute to DXP biosynthesis. It is known that the major polyamine produced by R. rubrum is spermidine25,26, which requires the organism to cope with the dead-end product MTA that is formed from SAM during spermidine biosynthesis. Since the majority of pigments in the purple-colored non-sulfur bacterium R. rubrum are carotenoid-based, we note that the biosynthetic shunt described here, would fit very well to the organism’s physiology because it allows the functional coupling of two biologically important processes in R. rubrum, polyamine biosynthesis and isoprenoid metabolism. As a matter of fact, carotenoid quantification experiments indicate up to 10% differences between aerobically grown R. rubrum wild type cells and MTA-isoprenoid shunt mutants (Supplementary Fig. 7). However, how much DXP exactly is synthesized via this metabolic shunt in R. rubrum remains to be investigated.
Phylogenetic analysis suggests that the MTA-isoprenoid shunt is not restricted to R. rubrum. R. rubrum RLP and related sequences (Supplementary Table 6) form a distinct branch in the cladogram that is well separated from RubisCOs type I–III, or other defined RLP groups2 (Fig. 1), indicating a similar physiological function. A detailed analysis of more than 30 genomes confirm that almost all organisms harboring a R. rubrum RLP homolog also show the genetic potential to reductively release methanethiol from MTA analogous to the reaction sequence proposed here (Supplementary Table 2). This is further supported by the observation that in many of these organisms, MTA-phosphorylase and MTR-1P isomerase, on the one hand, and RLP and cupin, on the other hand are encoded by the same genomic region (or represent protein fusions). However, in some cases, MTA-phosphorylase is functionally replaced by a 5′-methylthioribose kinase homolog, or (phospho)-hydrolytic enzymes indicating that the initial steps that produce MTR-1P (from MTA or a similar substrate) might differ slightly, as seen for the classical methionine salvage pathway11,27. Similarly, the genomes of Ochrobactrum, Thermotoga, Oceanithermus and Hoeflea, suggest some variation of the reaction sequence. Here, obvious cupin homologs are missing, although all other genes of the proposed pathway are clustered on the genome together with other genes (e.g., a conserved transketolase-like protein). For these organisms, it remains to be tested if methanethiol is indeed released during metabolism of MTR-1P (e.g by the transketolase-like protein) or whether the steps downstream of the RLP differ from the reductive release-reaction sequence proposed in this study.
We would like to note that LC-FTMS-metabolomics, as demonstrated here, is a powerful tool to elucidate microbial pathways and assign enzyme function on an organismal level, especially when potential substrates are not available and other methods such as transcriptomics and proteomics alone are inconclusive (e.g., in case of a non-essential, housekeeping pathway with otherwise low enzyme activities as shown here). In combination with classical knock-out methods, LC-FTMS metabolomics provide a synergistic approach to assign enzyme functions on a whole cell level, and future efforts will focus on developing our knock-out metabolomics method into a more systematic platform. In conclusion, LC-FTMS-metabolomics allows a mostly unbiased view into metabolic reactions in vivo, thereby identifying bona fide reactions even when not all (physiological) determinants or constraints are known (e.g., the unexpected involvement of a thiol-based reducing equivalent for the release of methanethiol).
Finally, the finding that RLPs of the R. rubrum group operate in an alternative MTA-degradation pathway adds another piece of information to the evolutionary puzzle of the biosphere’s most abundant protein, RubisCO. All RLPs characterized so far have been reported to be involved in sulfur metabolism, suggesting an interesting evolutionary link between sulfur and carbon metabolism. However, whether this evolutionary relationship is simply based on the fact that the substrates for RubisCO and RLPs are structurally related, or if there is a more general connection between sulfur metabolism and carbon fixation in evolution will be the object of ongoing discussions2,28–31.
For 1H-NMR on cell extracts, cells growing on minimal medium with sulfate or MTA as sulfur source (100 ml scale, OD578=0.5–0.8) were harvested by centrifugation (8,000×g, 10 min, 4 °C). Cells (0.3–0.5 g) were resuspended in 100 mM potassium phosphate in D2O (0.4–0.7 ml, pD 7.8) and lysed by sonication on ice (20–30×5 s pulses, 1/8” microtip horn, 15% intensity, level 3, Misonix Ultrasonic Sonicator XL2020). Cell debris was pelleted by centrifugation (14,000×g, 10 min, 4 °C), and the protein concentration in the supernatant was determined according to Bradford using BSA as standard32. In some cases, the cell extract was additionally exchanged against buffer in D2O by ultrafiltration-centrifugation using a 10 kDa exclusion membrane to remove excess traces of H2O. MgCl2 was added to a final concentration of 3–5 mM, and 1H-NMR spectra of cell extracts (0.75–1.0 ml, 0.5–1.0 mg total protein) were acquired on a Varian Unity Inova 500 NB spectrometer (Varian, Palo Alto, CA) before and after adding MTA to the NMR tube (0.7–1.0 mM final concentration) every 30 min over a time course of 12–16 hours at 30 °C (number of transients per spectrum=256, 17 min acquisition time). Formation of MTR-1P and MTRu-1P from MTA was confirmed by the (dis)appearance of characteristic signals known from authentic standards To determine formation rates of MTR-1P and MTRu-1P, the relative concentrations of both compounds compared to the absolute concentration of MTA (0.9–1.1 mM) were quantified via integration of the characteristic methylthio proton-signal of each compound (D2O/cell extract, 500 MHz, δ (in ppm) for the H3CS-group of MTA=2.07 s; δ for H3CS-group of MTR-1P=2.13 s; δ for H3CS-group of MTRu-1P=2.09 s).
Cells for metabolomics analysis were prepared from freshly grown cultures of R. rubrum wildtype and mutants (100 ml scale, OD578=0.5–0.8) by centrifugation (4,000×g, 10 min, 4 °C). Cell pellets were washed by resuspension in 25–40 ml minimal medium without sulfur source, followed by centrifugation and resuspension in 3–5 ml of minimal medium without sulfur source. Then, the OD578 of these cell suspensions was adjusted to 6.0 with minimal medium without sulfur source, and incubated for 10 min at room temperature (22–24 °C). Cell suspension aliquots of 1 ml were prepared in eppendorf tubes and pelleted by centrifugation (14,000×g, 5 min, 22–24 °C). The supernatant was discarded, and cell pellets were kept on ice until start of the feeding experiment (or frozen away for direct metabolite extraction).
The cell pellet aliquots on ice were resupended in 1 ml minimal medium without sulfur source (control samples), 1 ml minimal medium containing 1–2 mM MTA (feeding samples), or frozen directly in liquid nitrogen (t0 samples). Cells were incubated for 2, 10, or 20 min at 30 °C, before pelleting by centrifugation (14,000×g, 90 s, 4 °C). The supernatant was decanted by strongly flicking the eppendorf tube. Cell pellets were immediately frozen away in liquid nitrogen, and samples were stored at −80 °C until further use.
To extract metabolites, frozen cell pellets were resuspended in 0.375 mL 10 mM ammonium bicarbonate buffer (pH 9.2) containing 90% acetonitrile and then analysed immediately. LC-FTMS analysis was performed on the custom instrument described in the supplementary methods equipped with an Agilent 1200 HPLC system. Extracted metabolites were analyzed by injecting 100 μL of the sample onto a 2.1 X 150 mm Zic-HILIC column (Sequant) equilibrated with 10 mM ammonium bicarbonate buffer (pH 9.2) containing 90% acetonitrile (solvent B). Solvent consisted of 10 mM ammonium bicarbonate (pH 9.2). A linear gradient of 100%B to 40%B over 35 min then 40%B to 100%B in 10 min followed by a 15 min re-equilibration, at a flow rate 200 μL/min was used. All data were collected in negative profile mode at resolution 50,000 with full scan set to m/z 100–1000.
Data were analyzed using the software package SIEVE 1.3 (Vast Scientific). Default parameters were used except: max frames were set to 2000, threshold was set to 5000, and m/z tolerance was set to 0.001. Identification was performed using the Chemspider interface searched against the KEGG database. Peak lists were filtered to remove adducts and isotope peaks. Further filtering returned a peak list that showed significant change between the control and MTA fed samples (P value <0.01). The resulting peak list was exported to Microsoft Excel for relative quantitation using integrated intensities of the significant peaks. Manual analysis using the Qualbrowser application of Xcalibur (Thermo-Fisher Scientific) was performed on all automatically called significant peaks to remove missed isotopes, adducts, multimers, and erroneously called peaks. Peak identifications were corroborated using isotope pattern analysis and authentic standards as appropriate. Complementary data analysis was performed using the freely available software package XCMS33 and a newly developed in-house program that will be released elsewhere. XCMS analysis used the group, rector and fillPeaks and groupval functions. XCMS results were then analyzed using our in-house software. Briefly, the XCMS called peaks were further refined through deisotoping and removal of adducts taking into account multimers as well as canonical adducts. Peaks were further filtered by retention time. Peaks less than 3.5 min or greater than 35 min were removed from the sample sets. Peaks that were statistically different between samples were ranked using One-Way ANOVA. Only peaks with a p-value less than 0.01 were selected for further analysis. Isotopes and their relative abundance were also investigated to calculate the possible elemental compositions of the intermediates. Accurate mass of the predicted top three formulas was used to search databases with a mass tolerance of 2 ppm. Database searches were performed using the online interface modules of KEGG (http://www.genome.jp/kegg/)34, M E T L I N (http://metlin.scripps.edu/)35, and HMDB (http://www.hmdb.ca/)36. Search hits were compared with each other, and all analyses were manually validated.
Information on bacterial strains and cultivation conditions, fine chemicals and syntheses, heterologous expression and purification of enzymes, mutagenesis, enzymatic and whole cell assays, as well as proteomics and transcriptomics is available in Supplementary Methods.
T.J.E., B.S.E., and J.A.G. conceived and designed the experiments. T.J.E. performed the experiments with exception of metabolome analyses that were acquired by B.S.E., K.C., and B.M.W., as well as biochemical characterization of the cupin protein in vitro that was performed by B.S.E, and B.P.W. B.S.E., K.C., B.M.W., and J.V.S. developed the mass spectrometric platform and evaluated mass spectrometric data. J.S. and F.R.T. created and provided the rlp-and cupin-mutant strains of R. rubrum. B.P.W. and H.J.I. provided chemicals and recombinant enzymes for the synthesis of chemicals. T.J.E. and J.A.G. wrote the paper.
FN4Competing financial interests
The authors declare no competing financial interests.
This research was supported by a fellowship to T.J.E. from the Deutsche Forschungs-gemeinschaft (ER 646/1-1) and research grants from the National Institutes of Health (R01GM065155, R01GM095742, P01GM071790, and U54GM093342). We would like to thank John E. Cronan for critical comments, and Caitilin Deane and Taka Miyairi for excellent technical assistance. We also acknowledge Steven C. Almo and Brandan S. Hillerich (New York Structural Genomics Research Consortium; NYSGRC) for providing expression plasmids and purified cupin for in vitro assays.
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