The human pathogen Mycobacterium tuberculosis is the causative agent of tuberculosis resulting in over 1 million fatalities every year, despite decades of research into the development of new anti-TB compounds. Unlike most other organisms M. tuberculosis has six putative genes for epoxide hydrolases (EH) of the α/β-hydrolase family with little known about their individual substrates, suggesting functional significance for these genes to the organism. Due to their role in detoxification, M. tuberculosis EH’s have been identified as potential drug targets. Here, we demonstrate epoxide hydrolase activity of M. thermoresistibile epoxide hydrolase A (Mth-EphA) and report its crystal structure in complex with the inhibitor 1,3-diphenylurea at 2.0 Å resolution. Mth-EphA displays high sequence similarity to its orthologue from M. tuberculosis and generally high structural similarity to α/β-hydrolase EHs. The structure of the inhibitor bound complex reveals the geometry of the catalytic residues and the conformation of the inhibitor. Comparison to other EHs from mycobacteria allows insight into the active site plasticity with respect to substrate specificity. We speculate that mycobacterial EHs may have a narrow substrate specificity providing a potential explanation for the genetic repertoire of epoxide hydrolase genes in M. tuberculosis.
Infectious diseases pose a major threat to societies in the twenty-first century as many bacteria have managed to evolve mechanisms that protect them from antibiotics1. Of particular concern is infection with Mycobacterium tuberculosis (M. tuberculosis) the causative agent of tuberculosis, which caused approximately 10.4 million cases in 2017, resulting in 1.3 million deaths in HIV-negative patients. Alarmingly, in excess of 4% of the cases in 2017 were found to be multi-drug resistant2. In addition to this, there have been several reports of totally drug resistant tuberculosis in recent years3,4,5. In spite of decades of intense research simple, effective solutions to treat tuberculosis are still unavailable6. These facts demonstrate that it is of paramount importance to gain a more comprehensive understanding of the biological foundations of M. tuberculosis to be able to treat tuberculosis in the future.
Substantial insight into M. tuberculosis biology was provided by sequencing of its complete genome, which revealed that a comparably large fraction of all genes codes for enzymes involved in lipogenesis and lipolysis7,8. While epoxide hydrolases (EHs) are found in about 20% of all organisms with sequenced genomes, most of them occur in organisms with large genomes (> 8 Mb). The mycobacterial genome harbors less than 4 Mb but contains on average five epoxide hydrolases compared to approximately 2 found in other organisms. Since evolutionary pressure drives bacteria to deleting unneeded genes, this comparably large number of EHs supports the idea of functional significance of these enzymes to M. tuberculosis biology9. Initially, six putative copies of epoxide hydrolases ephA–ephF (EHs; E.C. 126.96.36.199; open reading frames Rv3617, Rv1938, Rv1124, Rv2214c, Rv3670 and Rv0134) could be identified7. Later another open reading frame (Rv2740) was shown to produce an atypical epoxide hydrolase (E.C. 188.8.131.52)10. At present, four of these genes have been confirmed to produce proteins with resulting enzymatic activity of an epoxide hydrolase (ephAthis work, ephB11,12, ephD13, ephG10). The idea to use mycobacterial EHs as potential drug targets was recently emphasized by screening of a large compound library in a whole cell phenotypic minimum inhibitory concentration (MIC) assay, which pointed towards EHs as the main target of the lead compound14.
EHs are essential enzymes that convert toxic epoxides to less reactive and more water soluble trans-dihydrodiols. They are generally implicated in detoxification of genotoxic epoxides but are also involved in more specialized processes like carbon catabolism and signal transduction. To date, three main classes of EHs have been identified; bacterial limonene EH (LEH), LTA4 hydrolases and α/β-hydrolase fold EH15. LEHs are essential for bacteria that use limonene as their only carbon source. The structural analyses of LEH from Rhodococcus erythropolis and an atypical EH from M. tuberculosis showed that these EHs do not belong to the family of α/β-hydrolases but rather consists of an α/β-barrel fold and follow a different reaction mechanism10,16. The second group EHs, the LTA4 hydrolases are Zn-dependent and show structural similarity to the bacterial protease thermolysin17. Similar to the bacterial LEHs, the LTA4 hydrolases display a specifically evolved active site and reaction mechanism15.
The majority of mycobacterial EHs have been predicted to be members of the α/β-hydrolase fold family, presenting the third and largest class of EHs. Significant insight into the reaction mechanism of this EH-family was gained by several crystal structures of bacterial and mammalian EHs18,19,20,21,22. The structures of the α/β-hydrolase family EHs can be divided into two subdomains; the catalytic ‘core-domain’ and the so-called ‘cap-domain’. The active site is located in a cleft between these two domains. The core domain contributes a conserved catalytic triad to the active site, while two strictly conserved tyrosine residues are located in the cap-domain. These tyrosine residues are suggested to affect epoxide polarization and facilitate ring opening23,24. The two-step reaction mechanism starts with an attack by the nucleophilic active site aspartate at one of the substrates epoxide carbons forming a covalent substrate-enzyme intermediate. Subsequently, a charge-relay pair between a general acid (aspartate/glutamate) and a general base histidine activates a water molecule. This leads to the hydrolysis of the covalent enzyme–substrate intermediate. A conserved histidine-glycine-X-proline (HGXP) motif that is generally found in α/β-hydrolases, together with the nitrogen atom of the residue following the nucleophile forms an oxyanion hole that is suggested to stabilize the intervening tetrahedral intermediate23,24,25,26,27. Computational evidence supports that this catalytic strategy is conserved for enzymes within this family28.
EHs of the α/β-hydrolase family are known to accept a broad spectrum of structurally diverse substrates. In mammals, the soluble EHs hydrolyze gem-di-, trans-di-, cis-di-, tri- and tetra-substituted epoxides, while the microsomal EHs hydrolyze mono- and cis- di-substituted epoxides. On a molecular level, this broad substrate spectrum could be explained by the nucleophile elbow, a sharp turn in the active site, which harbours the nucleophilic aspartate that is responsible for the initial substrate attack11,15,18,23,24. It has been suggested that an increased flexibility of this aspartate enables adaptation to the position of the substrate in the active site15. Due to the high structural similarity between mammalian and bacterial EHs, it would seem conceivable that mycobacterial α/β-hydrolase EHs show a similar versatility. However, the position of the nucleophilic aspartate and the other active site residues of M. tuberculosis epoxide hydrolase B (Mtb-EphB, Rv1938) remain unaltered in the inhibitor bound and ligand-free protein11.
In combination with the comparably large number of Ehs in mycobacteria this lets us speculate about an individual substrate selectivity, presumably targeting classes of different substrates9. In support of this hypothesis, the structure of Mtb-EphB has revealed a relatively small and hydrophobic active site and an altered substrate selectivity in comparison to mammalian or plant EHs11. However, our understanding of a particular active site geometry in relation to substrate specificity is limited by the available structural information, limited to Mtb-EphB, to date. Several EH inhibitors have not only shown antitubercular activity and low cytotoxicity but also to target several different EHs. However, these inhibitors have also targeted the human enzymes14. Therefore, in the design of epoxide hydrolase inhibitors for the treatment of TB, it is desirable to increase their specificity selecting only mycobacterial targets, which would be facilitated by structural knowledge of all mycobacterial EHs. From the six putative α/β-hydrolase EHs in M. tuberculosis only the structure of Mtb-EphB has been solved to date11. Although the crystallization of M. tuberculosis Epoxide hydrolase A (Mtb-EphA, Rv3617) has been reported, its limited X-ray diffraction prevented structure determination12. To enhance our structural understanding mycobacterial epoxide hydrolases, we have solved the crystal structure of the M. thermoresistibile Epoxide hydrolase A (Mth-EphA) in complex with a urea-based inhibitor at 2.0 Å resolution. The structure clearly displays an α/β-hydrolase EH fold but in comparison to other EHs shows substantial differences in the substrate binding channel.
Protein characterization and enzyme activity assay
A sequence comparison of epoxide hydrolase A from M. tuberculosis (Mtb-EphA) and its temperature tolerant relative Mycobacterium thermoresistibile (Mth-EphA) shows that the two orthologs share approximately 75% sequence identity. All residues suspected to be involved in catalysis are identical (Figure S1). This demonstrates that Mth-EphA may serve well as a model to understand the molecular details of Mtb-EphA. Consequently, the gene for Mth-EphA was cloned and expressed in E. coli, the recombinant protein was purified to homogeneity.
To qualitatively determine whether Mth-EphA has indeed epoxide hydrolase activity we incubated the protein with following compounds: cis-stilbene oxide (1), trans-stilbene oxide (2), or trans-1,3-diphenyl-2,3-epoxypropan-1-one (4) (Fig. 1) and analyzed its reaction products by liquid chromatography mass-spectrometry (LC–MS) (Table 1). Treatment of 1 or 2 with Mth-EphA did not reduce the concentration of any of those two compounds in the assay samples and did not give rise to hydrobenzoin (3) (Fig. S5–S7). However, treatment of 4 with Mth-EphA reduced the concentration of its adducts (H+, NH4+ and Na+, retention time 37.5 min) in the measured samples approximately to half of the initial values and gave rise to three signals with m/z values of 243Th, 260Th and 265Th, all with identical retention time of 15 min. We concluded that these molecular species must be three adducts (H+, NH4+ and Na+, respectively) of the chemical compound with molecular weight of 242 Da, which is characteristic to the hydroxylation product of 4, 2,3-dihydroxy-1,3-diphenyl-1-propanone (5) (Table 1 and Fig. S8–S11). The latter is commercially not available. Therefore, for fragmentation of those three molecular species (5-H+, 5-Na+, 5-NH4+) and the three adducts of 4 (4-H+, 4-Na+, 4-NH4+) the MRM parameters established for 4 have been used. The species 4-Na+ and 5-Na+ as expected did not give any measurable fragments because sodium adducts normally tend to produce very low fragmentation. The molecular species 4-H+, 4-NH4+, 5-H+ and 5-NH4+, all produced three fragments with m/z of 51Th, 77Th and 105Th (cf. Table 1, fragments 4-1, 4-2, 4-3, 5-1, 5-2, 5-3). While the first is characteristic for fragmentation of phenols, the second and third correspond to fragmentation results of substituted phenols. For the molecular species 5-H+ and 5-NH4+ fragments with m/z of 119Th and 225Th could be observed. The first species can be easily identified as 2-oxo-2-phenylethylium (5-4), while the second species (5-5) has an m/z value identical with 4-H+. In other words 5 showed neutral loss of water which is a typical fragmentation pattern of alcohols. A loss of a second molecule of water by fragmentation of the 5-5 would be conceivable if the 5-5 was an alcohol, too. But the putative product of such fragmentation with m/z 197Th (C15H11O1+) was not observed. Thus, we concluded that under neutral loss of one water molecule the diol (5) is converted to a dicarbonyl compound (5-5) in a way similar to the pinacol rearrangement. Therefore the 5-5 must be a protonated 1,3-diphenylpropanedione and not 1,3-diphenylhydroxypropanone.
In conclusion, the LC–MS data are consistent with 5 being 2,3-dihydroxy-1,3-diphenyl-1-propanone indicating that Mth-EphA can convert 4 to 5 under described reaction conditions. By contrast, the hydroxylation of the two other potential EH substrates 1 and 2 was not observed.
The purified protein was used in crystallization experiments which following optimization, yielded crystals diffracting to 2.0 Å resolution (Table 2, Figure S1). The structure was solved by molecular replacement using a homology model as template. Despite the challenging diffraction properties of the crystals, the data yielded an electron-density map with clearly interpretable features allowing accurate model building for residues 4–321 of the protein construct. All residues lie within allowed Ramachandran areas, with the exception of the active site residue Asp103. The strained conformation of Asp103 can likely be explained by its position at the tip of the nucleophilic elbow. Notably, Asp103 displays very well-defined electron density and its unfavorable conformation is held in position by interactions to the surrounding residues. Asp103 forms backbone hydrogen bonds to Ala106, Leu107 as well as Leu126 and its side chain carboxyl group contacts the backbone nitrogens of Phe35 and Trp104. Although four monomers were observed in the asymmetric unit, no significant dimer interface that would lead to the formation of a stable quaternary structure was determined in PISA analysis29.
This is consistent with native mass spectrometry (MS) analysis demonstrating that Mth-EphA is a monomer in solution (Figure S1). When sprayed from a nano-ESI (electrospray ionization) source the peaks appeared in a narrow charge state distribution with mainly + 10 and + 11 charges indicating a well-defined fold. A dissociation constant (KD) can be estimated from the relative peak intensities of apo Mth-EphA (100%) compared to Mth-EphA bound to 1,3-diphenylurea (DPU) (5%). However, the intensity ratios will not reflect the KD of such a hydrophobic interaction. Generally, non-polar interactions are poorly preserved in the gas phase and unspecific clustering rarely occurs. Detecting this interaction suggests that it is in fact specific, and that it would likely be much stronger in solution. Moreover, such a small hydrophobic ligand would be unlikely to detect at all if not buried inside the molecule30.
The overall structure of Mth-EphA clearly displays the globular fold of the α/β-hydrolase EHs. It is separated into two domains; the α/β-hydrolase core-domain (residues 1–136 and 247–321) with its central, eight-stranded β–sheet and the all-α-helical cap-domain (residues 137–246) (Fig. 2). The interface between cap-domain and core-domain harbors the active site of Mth-EphA, with the conserved residues of the catalytic triad (Asp103, His297 and Asp268) and the epoxide polarizing tyrosines (Tyr153, Tyr238) (Fig. 2). The cap-domain closes over the core-domain leaving space for a characteristic ‘L’-shaped tunnel with a hydrophobic interior (Fig. 2). The tunnel has an overall length of approximately 30 Å and bulky cavities close to its two distinct solvent openings, with radii of 2.7 Å and 3.4 Å, respectively (Figure S2). However, at its center, in proximity to the active site residues, it shows a constriction with a radius of only 1.2 Å. This constriction is imposed by three hydrophobic residues (Leu107, Met241, Met274) and presumably influences the substrate selection by Mth-EphA. A surface charge calculation shows a generally acidic surface for the cap-domain of Mth-EphA, while the surface charges at the core-domain are less pronounced. Interestingly, the two openings to the substrate-channel display opposite charges. While one opening has a strongly acidic surrounding the other shows clear alkaline properties (Fig. 2). It is conceivable that these properties influence substrate selection or guide substrate orientation and binding.
The previously established EH inhibitor 1,3-diphenylurea was co-crystallized with Mth-EphA. The inhibitor is deeply buried within the substrate tunnel, where it binds to the conserved active site residues (Fig. 3). The conformation of the inhibitor binding could be unambiguously determined from the electron density maps. While both of the amine nitrogens form hydrogen bonds with Asp103, the phenyl groups are stabilized by van der Waals interactions (Phe35, Met178, Leu182, Phe200, Trp298 and Trp104, Leu107, Ile154, Met241). The carbonyl oxygen of the inhibitor is hydrogen bonded by Tyr153 and Tyr238 mimicking the position of the epoxide oxygen. Interestingly, the inhibitor adopts a slightly bent conformation with the carbonyl group and both phenyl-rings oriented towards Tyr238. In proximity of Asp103 and His297 a water molecule shows electron density and is stabilized by hydrogen bonds to the side chains of those residues, to Glu39 as well as to the main chain of Phe35 (Fig. 3).
M. thermoresistibile epoxide hydrolase A has high sequence similarity to its orthologue from M. tuberculosis and its crystal structure described here displays overall high structural similarity to α/β-hydrolase EHs. To gain insight into its substrate binding properties and shed light on its potential substrate specificity, we compare its substrate channel with that of another bacterial EH and the human orthologue. The structure of Mth-EphA presented here can be superimposed onto the structures of Mtb-EphB (2ZJF), to the EH from Agrobacterium radiobacter (1EHY) and to the catalytic domain of human soluble epoxide hydrolase (sEH; 1S8O) with an average r.m.s.d. of less than 0.5 Å. Moreover, the global similarity of the EHs is not limited to their main chains but also extends to the catalytic residues in the active site, which directly overlap upon superposition (Fig. 4).
However, in spite of the conserved active site conformation, substantial differences in the substrate channels can be observed. Mth-EphA features a wide double cavity that is connected by a narrow constriction at its center (Figs. 2, 4, Figure S2 and S3). The channel has two major openings to the solvent that exhibit opposite surface charges, while the other EHs compared here do not feature opposite charges at their active site entry sites. Mtb-EphB, which shares 40% sequence identity with Mth-EphA, on the other hand has a much narrower substrate channel with only two minor connections to the solvent. Moreover, upon superposition of the structures it is evident that the individual substrate channels not only have different shapes and sizes but also propagate along different directions.
Similar to the mycobacterial EHs, the human sEH channel also has two openings to the solvent. However, clearly distinct from the mycobacterial EHs, the channel of the human orthologue appears to be wide enough to accept a variety of different and bulky substrates. This is consistent with its general versatility accepting differentially substituted epoxy fatty acids as substrates16,23,31. In contrast to the former structures, the EH from A. radiobacter has only one large opening on its surface and a shallow connection to the active site that is not fully shielded from the solvent (Fig. 4, Figure S4). It appears to be better suited to accommodate smaller substrates with epoxides on terminal positions consistent with its primary, natural substrate epichlorohydrin32,33.
Unfortunately, to the best of our knowledge the actual substrate specificity of mycobacterial EHs are unknown. However, a comparison of the affinities of inhibitors for human sHE and Mtb-EphB indicates substantial differences between the two enzymes. Both of them can bind smaller inhibitors like 1,3-diphenylurea with high affinity. In consistence with its narrow substrate channels, Mtb-EphB shows much lower affinity to those inhibitors that exhibit long or bulky side-chains11. This suggests that its natural substrates could also be smaller molecules. The substrate channel of Mth-EphA is clearly distinct from the one in Mtb-EphB, showing two bulky cavities, a constriction at its center and highly polar entry sites (Fig. 2). It is conceivable that these features could play a role in substrate orientation and selection. In line with these findings Mtb-EphB shows activity against both cis- and trans-stilbene oxide while Mth-EphA did not show any activity against either of the compounds in our assay11. In summary, the properties of the active site channels as well as the results of our activity assay support the view that the comparably large genetic repertoire in mycobacterial epoxide hydrolases may be related to the substrate specificity of the individual enzymes. In line with this a sequence alignment reveals that the residues that line the substrate channel predominantly map to the most variable parts of the EHs, that is the α-helical cap-domain (Fig. 5). Similar to Mth-EphA and Mtb-EphB, the remaining mycobacterial EHs also show substantial sequence variability in their putative substrate channel locations. This further supports our view that mycobacterial epoxide hydrolases may have varying substrate specificities. Thus, we speculate that the large genetic repertoire of EHs in M. tuberculosis may have evolved to address different substrate classes.
The nature of the substrate of EHs is likely to have important kinetic consequences: human soluble EHs are able to process a large number of structurally diverse substrates following a 2-step reaction mechanism whereas the LEH from Rhodococcus erythropolis has a very narrow substrate specificity and enantio-selectivity. However, this narrow specificity is linked to a high turnover number of its main substrate maintaining its efficient hydrolysis15,16,34,35. By analogy, it is conceivable that a narrow substrate specificity of mycobacterial EHs could be linked to higher turnover rates. Therefore, the evolution of a large number of mycobacterial EHs could be an adaptation for the efficient hydrolysis of different substrate classes.
This is in good agreement with other physiological properties of M. tuberculosis. Since a large fraction of its genome is dedicated to the lipid metabolism it is reasonable to assume that it also requires an increased number of lipid-modifying enzymes. Moreover, the degradation of host cell lipids is vital to M. tuberculosis, as they serve as precursors for metabolic processes and are utilized as components of the mycobacterial cell wall7. This hypothesis gains support from recent findings that show up-regulated expression of epoxygenases in human macrophages, the natural habitat of M. tuberculosis36,37. Thus, it is conceivable that due to its genetic repertoire in EHs, M. tuberculosis is able to exploit the modified fatty acids present in human macrophages. Moreover, epoxygenases were also recently implicated in infection with intracellular bacteria underlining the potential importance for mycobacterial EHs during infection38.
Clearly, further research is required to fully understand the importance of EHs and the role they play during mycobacterial infections. Their overall structure is highly similar to the human soluble EH rendering an inhibitor design that targets the catalytic residues a challenging task. However, the structure of Mth-EphA described here furthers our understanding of the mechanism by which EHs might achieve substrate specificity and points to new opportunities for modulation of their activity. Further crystal structures of the remaining EHs (EphC-F) would add to our understanding of the nuances of mycobacterial EHs and facilitate design of EH-inhibitors that target other features of the proteins. The subtype specific substrate channels appear to be an interesting goal for future studies—not only limited to inhibitor design but also to better understand mycobacterial EH substrate specificity and thus their interaction with the host cell.
The gene encoding Mycobacterium thermoresistibile epoxide hydrolase A (Mth-EphA) (gi 490022613) was cloned into the pETM-11 vector (EMBL); protein expression was conducted in Escherichia coli Rosetta 2 (DE3) in LB medium at 20 °C for 18 h. The Mth-EphA construct used in this study contained all amino acids of the 321-residue protein. At the N-terminus it contained 4 additional residues (Gly-Ala-Met-Ala) linked to a TEV protease cleavage site and His6-tag. The His6-fusion protein was purified via affinity chromatography on a Ni–NTA resin (Quiagen) following the manufacturer’s instructions (50 mM Tris/HCl pH 7.5, 300 mM NaCl, 5% (v/v) glycerol). The His tag was removed by addition of TEV protease and dialysis at 4 °C for 18 h (50 mM Tris/HCl pH 7.5, 50 mM NaCl, 5% (v/v) glycerol). To remove the cleaved His6-tag and the TEV protease the solution was further purified via a MonoQ 10/100 ion exchange column (50 mM Tris/HCl pH 7.5, 5% (v/v) glycerol, 50–300 mM NaCl). EphA was further purified by Superdex S-75 size exclusion chromatography (50 mM Tris/HCl pH 7.5, 150 mM NaCl). Protein purity is not only reflected in a sharp, mono-dispersed elution profile in size exclusion chromatography but also in clear bands on SDS–polyacrylamide gels (Figure S1). Purified EphA was concentrated to 18 mg/ml and stored at − 80°°C until further use.
Native mass spectrometry (MS)
Purified Mth-EphA was exchanged into 150 mM ammonium acetate (AmAc) (PN431311, 99.99% purity, Sigma-Aldrich, MO, USA), pH 7.5, via centrifugal filter units (Vivaspin 500, MWCO 10,000, Sartorius, Germany) at 4 °C. The near physiological conditions allow on one hand preservation of the native fold of the protein and on the other hand prevent adducts by nano-ESI. For binding experiments a 500 mM DPU stock in DMSO was diluted 50:1 in 150 mM AmAc in order to produce a saturated solution, considering the maximum DPU solubility in aqueous solutions of 710 µM/L (The Merck Index. 9th ed. Rahway, New Jersey: Merck & Co., Inc., 1976., p. 227) with and without 10% (v/v) butanediol, since it was also used for crystallization. Prior to measurements the inhibitor mix was diluted and incubated with EphA, resulting in 6 μM EphA, 71 μM DPU and 0.2% DMSO. Native MS was carried out in positive ion mode on a QToF 2 (Micromass/Waters, UK) modified for high masses (MS Vision, the Netherlands)39. The gas pressures were 10 mbar in the source region and 1.2 × 10–2 mbar Argon in the collision cell. Raw data were calibrated with CsI (25 mg/mL) and analyzed using MassLynx (Waters). Peak deconvolution and determination of relative intensity was performed using UniDec40.
LC–MS based enzyme activity assay
Stock solutions of cis-stilbene oxide (1), trans-stilbene oxide (2), hydrobenzoin (1,2-diphenyl-1,2-ethandiol) (3), trans-1,3-diphenyl-2,3-epoxypropane-1-one (4) were prepared in methanol LC–MS grade (each 20 mM) and kept at − 80 °C. Assay and control samples were prepared as follows: To 200 µl of the assay buffer (25 mM Tris-formic acid pH 7.2) 4 µl of one of the potential EH substrates (1, 2 or 4, final concentration in the assay 400 µM) was added. The reaction in the assay samples was started by addition of 0.5 µl of 20 µM enzyme solution (final concentration 0.025 µM). To control samples no enzyme was added. The assay and control a samples were incubated 60 min at 30 °C. Thereafter the samples were chilled on ice for 3 min and the reaction was quenched by addition of 800 µl of ice-cold methanol. After incubation on ice for 10 min the samples were centrifuged 30 min, 13,000 rpm, 0 °C. The supernatant was collected and stored at − 80 °C. The supernatant samples were analyzed on HPLC1200 (Agilent) equipped with PRP C18 column (150 mm × 2.1 mm, Hamilton) and coupled to API4000 Q-Trap Triple Quad mass spectrometer (SCIEX). Mobile phase A was 3 mM ammonium formate in water:methanol (1:1, v/v), mobile phase B was 3 mM ammonium formate in water:methanol (1:995, v/v). Aliquots (20 µl) were injected onto the column equilibrated with the mobile phase A. The column was developed with a gradient of the mobile phase A: 100%, at 0 min; 0% at 10 min; 0% at 45 min; 100%, at 46 min; 100%, at 70 min. The flow rate was 200 µL/min. MRM transition parameters (electrospray ionization, positive mode) for four available standard compounds were optimized using the Compound Optimization tool of the software Analyst (SCIEX). The m/z values, transition parameters and chemical formula of five compounds as well as their most populated fragmentation products are shown in the Table 1. The MRM chromatograms are shown in the supplemental material (Fig. S5–S11).
Mth-EphA displayed high sensitivity towards DMSO. Thus, an inhibitor complex was generated by diluting a 1,3-diphenylurea solution (100 mM in 100% DMSO) 1:50 (v/v) with the protein solution, the resulting precipitate was removed by centrifugation, the supernatant was used for crystallization trials. Mth-EphA crystallized in multiple conditions, however, best diffracting crystals were only obtained in presence of low concentrations of 2,3-butanediol (1–3% v/v). Crystals were grown at 18 °C in sitting drop vapour diffusion plates combining equal volumes of precipitant (0.1 M BisTris pH 7.5; 2.15 M (NH4)2SO4; 4.5% (v/v) PEG 400; 1–3% (v/v) 2,3-butanediol) and the protein solution. The crystals appeared infrequently, as thin and often coadunate plates within 2–3 weeks and grew to a size of approximately 100 × 80 × 10 µm (Fig. S1). Crystals were cryo-protected by soaking in precipitant solution containing additionally 12% (v/v) 2,3-butanediol. Crystals were flash frozen in liquid nitrogen prior to data collection.
X-ray data collection was performed at 100 K; diffraction images were collected at beamline ID30A-2 at ESRF, Grenoble, using the automated MASSIF data collection program41,42. Diffraction images were indexed, integrated and scaled using XDS and XSCALE, respectively43,44. Initial indexing of the diffraction patterns indicated an orthorhombic space group. However, analysis with PHENIX.XTRIAGE revealed a strong off-origin Patterson peak of ~ 56% origin intensity indicating pseudo-translational symmetry45. Moreover, it also revealed that the data are twinned by pseudo-merohedry (α ~ 33%; twin law h, -k, -l), which was later accounted for during structure refinement. These features suggested a lower symmetry space group, which was confirmed by an analysis with ZANUDA46. The crystals obtained in this study belonged to space group P21 (a = 61.8, b = 105, c = 108.9; α, β, γ = 90°) with four monomers in the asymmetric unit and diffracted up to a resolution of 2 Å. The structure was solved by molecular replacement (PHASER) using a homology model generated with the PHYRE2 server47,48. Model building was performed in COOT49. Coordinates were refined to reasonable stereochemistry using PHENIX.REFINE (Table 2)45. Alternating steps of refinement and structure adjustments were performed until the R-values converged. The structure was validated using MOLPROBITY50. It was refined to Rwork and Rfree values of 20.86% and 25.08%, respectively (Table 2). All Mth-EphA monomers can be superimposed to each other with an r.m.s.d. of less than 0.3 Å, demonstrating their structural equivalence. Refined coordinates were deposited in the RCSB as entry 5CW2.
Structure and sequence comparison
Protein sequences were derived from Tuberculist and aligned using TCOFFEE51,52. Sequence alignments were subsequently visualized using ESPRIPT253. Structure analysis was conducted using tools from the CCP4 suite as well as using software from the PHENIX package45,54. Substrate tunnels were calculated using the CAVER3.0 plugin to PYMOL. After superimposition of the individual structures the carbonyl oxygen from the 1,3-diphenylurea inhibitor was used as a common starting point, using default values for optimization. The probe radius was set to 1, the shell depth to 4 and the number of approximating balls to 20 for all protein structures. The shell radius and the clustering threshold were chosen individually to retrieve the most prominent tunnels (shell radius/clustering threshold: 1S8O-4/7; 1EHY-4/3.5; 2ZJF-3/3.5; Mth-EphA-3/3.5)55. Overlapping tunnels have been merged for visualization.
All molecular images were generated in PYMOL (Schrödinger LLC).
Coordinates and structure factors have been deposited in the Protein Data Bank under accession codes 5CW2.
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We are indebted to our colleagues Vivian Pogenberg and Annabel Parret for their continuous support, helpful discussions and critical reading of the manuscript. Moreover, we would like to thank the beamline staff of ID-30 from ESRF for their support during data collection.
Open Access funding enabled and organized by Projekt DEAL. This work was supported by an BMBF ERA-NET Grant Pathogenomic GeMoA to M.W. with Reference Number 0315908. The Heinrich Pette Institute, Leibniz Institute for Experimental Virology is supported by the Free and Hanseatic City of Hamburg and the Federal Ministry of Health. BK and CU are funded by the Leibniz Association through SAW-2014-HPI-4 Grant. This work was supported by the Max Planck Society, the Joachim Herz Foundation (Biomedical Physics of Infection) and the Excellence Cluster “CUI: Advanced Imaging of Matter” of the Deutsche Forschungsgemeinschaft (DFG), EXC 2056, project ID 390715994.
The authors declare no competing interests.
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Schulz, E.C., Henderson, S.R., Illarionov, B. et al. The crystal structure of mycobacterial epoxide hydrolase A. Sci Rep 10, 16539 (2020). https://doi.org/10.1038/s41598-020-73452-y
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