A major constraint for developing new anti-tuberculosis drugs is the limited number of validated targets that allow eradication of persistent infections. Here, we uncover a vulnerable component of Mycobacterium tuberculosis (Mtb) persistence metabolism, the aspartate pathway. Rapid death of threonine and homoserine auxotrophs points to a distinct susceptibility of Mtb to inhibition of this pathway. Combinatorial metabolomic and transcriptomic analysis reveals that inability to produce threonine leads to deregulation of aspartate kinase, causing flux imbalance and lysine and DAP accumulation. Mtb’s adaptive response to this metabolic stress involves a relief valve-like mechanism combining lysine export and catabolism via aminoadipate. We present evidence that inhibition of the aspartate pathway at different branch-point enzymes leads to clearance of chronic infections. Together these findings demonstrate that the aspartate pathway in Mtb relies on a combination of metabolic control mechanisms, is required for persistence, and represents a target space for anti-tuberculosis drug development.
Mycobacterium tuberculosis (Mtb), the causative agent of tuberculosis (TB), is the deadliest pathogen worldwide, with 1.8 million deaths in 2016, and is the source of severe societal and economic burdens1. Mycobacterium tuberculosis is able to establish a devastating chronic infection in humans, where it can withstand host adaptive immunity and survive in granulomas, a phase commonly referred to as persistence. Many drugs are ineffective during persistence, most likely due to reduced penetrance into the devascularized granuloma environment2 and enrichment of phenotypically drug-tolerant cells. As a result, treatment regimens require a lengthy 6-months of combination therapy to clear the infection, which greatly increases the risk of antibiotic resistance acquisition1,3.
Recent efforts to target Mtb during persistence have focused on inhibiting previously ignored metabolic pathways4,5. Several studies have demonstrated that central carbon metabolism (CCM) is required during persistence, and several targets have been identified as essential in both acute and chronic infections in mice4,5,6,7,8,9,10,11. Importantly, biosynthetic pathways that utilize TCA cycle intermediates, such as amino acid biosynthesis, are also required for Mtb survival12. However, none of the amino acid biosynthetic pathways of Mtb have yet been shown to be essential during chronic infection and it is largely unknown if such building blocks can be scavenged from the host during persistence.
We recently reported that methionine biosynthesis in Mtb is required to establish infections in immunocompetent and immunocompromised mice13. Methionine, along with isoleucine, threonine, and lysine make up the family of essential amino acids synthesized from aspartate via the aspartate pathway. This pathway is also involved in the biosynthesis of the peptidoglycan building block, diaminopimelate (DAP), and the cofactor, S-adenosyl methionine (SAM); both of which are required for survival in mycobacteria13,14. Because of its branched nature and pivotal role in essential cellular processes (cell wall biosynthesis, translation, and one-carbon metabolism), metabolic regulation of the aspartate pathway is likely important to meet precursor requirements during growth and persistence in the host15.
The apparent essentiality of the numerous metabolic products and absence of the aspartate pathway in humans and animals15 led us to investigate the effects of inhibition of the aspartate pathway in Mtb and its requirement during persistence in the host. We hypothesized that disruption of the aspartate pathway leads to a metabolic imbalance and eventual collapse of this essential biosynthetic network. To investigate this, we employed a combinatorial approach of mycobacterial genetics, transcriptomics, metabolomics, biochemical analysis, and animal experiments. Here, we show that both homoserine auxotrophy (∆thrA) and threonine auxotrophy (∆thrB) are bactericidal, and that methionine and threonine are jointly required for survival and persistence. Transcriptomic and metabolomic studies revealed that threonine starvation leads to an unexpected accumulation of lysine, which the cell responds to by activating lysine export and a mycobacteria-specific degradation pathway. Finally, we demonstrate the absolute requirement of the branch-point enzymes homoserine dehydrogenase (ThrA, Rv1294) and homoserine transacetylase (MetX, formerly known as MetA, Rv3341) in both acute and chronic tuberculosis infections. Taken together our work identifies and characterizes a vulnerable component of Mtb’s persistence metabolism with its metabolic control mechanism and puts it on the map for drug discovery.
Threonine and homoserine auxotrophy are bactericidal
The aspartate pathway produces essential proteinogenic amino acids threonine, methionine, lysine, and isoleucine, the co-factor S-adenosyl methionine, and the cell wall component diaminopimelate. To dissect the individual contributions of pathway branches to metabolic homeostasis and pathogen survival, we attempted to delete selected branch-point enzymes to create auxotrophic strains in Mtb. These auxotrophic strains could then be used to study metabolic alterations in vitro and serve as metabolic probes in vivo. We have previously shown that MetX (formerly known as MetA), a homoserine transacetylase that converts homoserine to O-acetyl-L-homoserine, is essential for Mtb survival13. Upstream of MetX lies an important branch point of the aspartate pathway because homoserine is needed for both threonine and methionine biosynthesis (Fig. 1a). In order to dissect the effects of combined methionine/threonine and single threonine or methionine auxotrophy, we made null deletion mutants of homoserine dehydrogenase (ThrA) and homoserine kinase (ThrB) in Mtb H37Rv, leading to the mutant strains ∆thrA and ∆thrB, respectively. Deletion of thrB yielded a threonine auxotroph (Fig. 1b), which was killed rapidly in vitro in the absence of threonine supplementation (Fig. 1c). Death in this mutant could not be rescued by addition of isoleucine. Deletion of thrA was bactericidal and could be rescued by either the addition of homoserine or by a combination of methionine and threonine (Fig. 1d). Interestingly, the addition of either methionine or threonine alone in ∆thrA led to a statistically significant slow-down of cell killing (Fig. 1e).
Threonine auxotrophy leads to accumulation of lysine and catabolites
We next sought to elucidate the cellular consequences to inhibition at the threonine- homoserine-methionine branchpoint. We employed a combinatorial transcriptomic and metabolomics approach. mRNA transcript levels of the ∆thrB and ∆thrA mutant strains were measured by RNA-seq and microarray analysis, respectively, in time-course experiments in growth media lacking the amino acids required for survival (Fig. 2). The ∆thrB and ∆thrA strains have an expression profile similar to that previously observed in methionine starvation (Supplementary Data 2)13 and general nutrient starvation (Supplementary Data 2)16, as evidenced by the downregulation of lipid biosynthesis and respiration-related genes, and upregulation of pyruvate and succinate metabolism (Fig. 2). However, there were also significant differences in gene expression that indicated killing by threonine and homoserine auxotrophy occurs via a mechanism distinct from that mediated by methionine or general starvation13,16. Threonine and homoserine auxotrophy each led to a particularly strong and early (within 2 days) response (upregulation) in redox stress gene expression (Fig. 2). The strongest changes were observed in genes involved in lysine degradation and export pathways. The third-most upregulated gene (8-fold) was the lysine-ε aminotransferase, lat (Rv3290c) (Fig. 2), which catalyzes degradation of lysine to α-aminoadipic acid semialdehyde (Fig. 1a). The lat gene has been identified as a persistence-related gene in Mtb and M. smegmatis16,17,18. The concurrent upregulation of pcd (Rv3293) (Fig. 2), which further degrades α-aminoadipic acid semialdehyde to α-aminoadipate, and Rv1986, a probable lysine exporter19, suggests a general upregulation in lysine disposal pathways.
To investigate if these substantial transcriptional changes also translate into metabolic changes, we characterized the intracellular and extracellular metabolomes by ultra-performance liquid chromatography-mass spectrometry (UPLC-MS). In accordance with the upregulation of genes for lysine disposal, the ∆thrA mutant in media lacking homoserine displayed a significant increase (up to 100-fold) of all identifiable metabolites in the lysine biosynthesis pathway (Fig. 3a). Diaminopimelate, lysine, α-aminoadipate, and N-acetylysine were all found in at least 10-fold greater abundance after 24 h of starvation of the ∆thrA mutant (Fig. 3a). Furthermore, lysine, but not other pathway intermediates, was found to accumulate extracellularly (Fig. 3b), suggesting increased activity of a lysine exporter. Over a period of 4 days the extracellular concentration of lysine increased to 160 µM after which it stayed constant (Supplementary Fig. 2). Analysis of the metabolomic response of threonine auxotrophy alone (Mtb ∆thrB) showed a similar pattern of intracellular metabolite abundances (Fig. 4), but in addition, Mtb ∆thrB also accumulated homoserine (Supplementary Fig. 3), the adduct of the thrB encoded threonine kinase (Fig. 1a), which nicely confirms the metabolic block at ThrB. In line with this homoserine accumulation, we observed increased expression of metX (Fig. 2b). Lysine export was also observed in the ∆thrB strain, albeit at a reduced rate compared to ∆thrA (Supplementary Fig. 4), which fits with the fact that carbon rerouting in ∆thrB occurs not only toward lysine but also homoserine. Homoserine was proposed to be toxic to M. tuberculosis20, and we have confirmed its toxicity for the MTB Complex strain M. bovis BCG (Supplementary Fig. 5). We observed an adverse role of homoserine but not threonine on growth of M. bovis BCG at concentrations above 50 µg/ml (Supplementary Fig. 5), which is in excellent agreement with the work published earlier20. These findings reveal accumulation of lysine, and homoserine in ∆thrB, that the cells attempt to manage by carbon-rerouting, lysine export and degradation. The lysine overload was particularly surprising given that most bacteria employ a lysine feedback loop that involves allosteric inhibition of aspartate kinase by lysine21,22,23,24,25,26,27.
Threonine is the main feedback regulator of Mtb’s aspartate pathway
Next, we wanted to understand at a regulatory level, how inhibition of ThrA or ThrB could lead to increased lysine production. Aspartate kinase (AK) encoded by ask (Rv3709c) catalyzes the first committed step in the aspartate pathway, converting aspartate to aspartyl phosphate (Fig. 1). In Escherichia coli, there are three AK isoforms that are separately sensitive to feedback regulation by threonine, lysine/leucine, or methionine, respectively21,23,24. The actinomycete Corynebacterium glutamicum regulates the aspartate pathway via a single AK that is feedback inhibited by lysine and threonine, and transcriptional repression of homoserine dehydrogenase (thrA) by methionine22,26. In M. tuberculosis, purified AK has been shown to be sensitive to threonine but not lysine27, yet no other amino acids (e.g., methionine or homoserine) were tested nor was it investigated if these results translated to whole-cell physiology. Methionine and SAM biosynthesis in Mtb are likely regulated at the transcriptional level13,28. Consequently, addition of threonine should reverse lysine accumulation in Mtb ∆thrA. Indeed, threonine was capable of decreasing intracellular lysine accumulation, causing a concomitant accumulation of aspartate (Fig. 3a). Furthermore, addition of methionine as a control, caused no change in lysine pathway metabolites (Fig. 4), indicating that the loss of threonine is the major driver for overproduction of lysine. This argues that L-threonine inhibition of AK is likely a primary metabolic control mechanism of the aspartate pathway.
A lysine exporter responds to disruptions in lysine homeostasis
We next investigated the unexpected export of lysine as an alternative mechanism to cope with lysine overload in the cell. Our transcriptomic analysis of the ∆thrA and ∆thrB mutants showed a strong upregulation of a putative lysine exporter Rv1986 and arginine biosynthesis genes (Fig. 2a, b). Moreover, metabolomic data demonstrates that intracellular accumulation of Lys leads to export of both lysine and arginine (Arg) (Fig. 5a) but not other amino acids or metabolites (Supplementary Fig. 6). It has been shown in C. glutamicum that lysine accumulation is toxic, and that export of both Lys and Arg is carried out by the exporter LysE29,30. A bioinformatic analysis showed that Mtb encodes several proteins with homology to LysE of C. glutamicum, yet only Rv1986 is located adjacent to its canonical transcriptional regulator LysG (Rv1985c) (Fig. 5b)19. Hence, we hypothesized that Rv1986 serves the purpose of an overflow mechanism to prevent intracellular lysine overload. To test the role of LysE in amino acid export of Mtb, we measured the ability of Mtb to export toxic amino acid analogs in the presence and absence of the LysE exporter. This is a commonly used strategy to characterize amino acid exporters in whole cells31. We deleted the genes lysE (Rv1986) and lysG (Rv1985c) in Mtb H37Rv, resulting in mutants ∆lysE and ∆lysG. Using these strains, we determined the minimum inhibitory concentration (MIC) of toxic amino acid analogs of lysine (2,6-diaminohex-4-ynoic acid), arginine (canavanine) and histidine (ß-2-Thiazolyl-DL-alanine) (Fig. 5c, d, e). These compounds (Supplementary Fig. 1) have previously been shown to be toxic analogs in other bacteria and act as substrates for their cognate amino acid exporters32,33,34. Toxicity arises from their aberrant incorporation into proteins during translation, and deletion of their analogs’ exporters should increase susceptibility (Fig. 5b). Indeed, we found that deletion of both lysE and lysG resulted in a greater than 10-fold reduction in the MIC of canavanine and 2,6-diaminohex-4-ynoic acid (Fig. 5c, d), but there was no change in the MIC of the histidine analog control (Fig. 5e). The lysE phenotype was rescued when genetically complemented (Fig. 5c, d) or when the cognate amino acid (e.g., arginine) was added as a competitive substrate (Supplementary Fig. 7). The results demonstrate that LysE exports lysine and arginine as predicted by its homology and similarity (32% identity determined by Basic Local Alignment Search Tool (BLAST)) to the C. glutamicum LysE permease and that LysG is the activator of LysE under the conditions tested (Fig. 5). We also found evidence that lysine disposal is relevant in Mtb during growth in standard growth medium under non-auxotrophic conditions. During the transition from exponential to stationary phase, lysine and aminoadipate are elevated in wild-type Mtb H37Rv (Supplementary Fig. 8) and the lysE deletion mutant shows a significant growth retardation under these conditions (Supplementary Fig. 9).
Taken together, these data indicate that Mtb utilizes lysine export and degradation pathways as a metabolic relief valve to prevent disruption of aspartate pathway homeostasis and maintain essential precursor production. Such a metabolic mechanism to maintain precursor availability for growth and survival is unprecedented in M. tuberculosis. It is tempting to speculate that prevention of lysine export, could synergize with inhibition of threonine production, and could be exploited to enhance bactericidal activity. To test this notion, we attempted to construct a double deletion strain ∆thrA∆lysE. However, multiple attempts were unsuccessful pointing to a synthetic lethal interaction between these two pathways.
Aspartate pathway enzymes are required during chronic infections
Given the potent bactericidal phenotypes observed in several auxotrophs in vitro, we next evaluated the need for aspartate family amino acid biosynthesis during host infection. We first tested the ability of the threonine/methionine auxtotroph Mtb ∆thrA to establish an infection in immunocompetent (C57BL/6)) and immunocompromised (SCID) mice via aerosol infection. Similar to ∆metX13, we found that ∆thrA mutant was incapable of establishing an infection in either C57BL/6 (Supplementary Fig. 10a, b) or SCID mice (Supplementary Fig. 10c, d). To test whether threonine auxotrophy alone prevents the establishment of infection, we also tested Mtb ∆thrB in C57BL/6 and found this strain to be avirulent too (Supplementary Fig. 11). However, as Mtb can maintain a persistent infection it is also necessary to test target vulnerability during an established, chronic infection35. As specific target inhibitors are not yet available, a genetic approach was employed. We constructed conditional knockdowns (cKD) of ThrA (∆thrA-DUC) and MetX (∆metX-DUC), using the tetracycline-induced Dual-Control (DUC) system35. Both constructs are transcriptionally regulated by an anhydrotetracycline (atc) -inducible transcriptional repressor (T38), and are simultaneously repressed by atc-induced proteolytic degradation (DUC)36,37. The knockdown efficiency was validated in vitro by measuring the effect of increasing concentrations of atc on growth of the recombinant strains in culture broth media (Fig. 6a, e). Growth of the DUC strains in medium without atc was indistinguishable from the parental strain, demonstrating genetic complementation to WT levels (Supplementary Fig. 12a). While the parental H37Rv strain showed no sensitivity to atc (Supplementary Fig. 12b), growth was inhibited in both knockdown strains (Fig. 6a, b). Next we tested the vulnerability of Mtb to inhibition of these enzymes during different stages of infection in C57Bl/6 mice. Cohorts of each infection group were started on doxycycline at 0, 1, 3, or 6 weeks after infection, which allowed us to study the in vivo essentiality of these enzymes during both the acute and chronic stages of infection (Fig. 6b, f). For both cKD strains, administration of doxycycline immediately after infection resulted in a total bacterial clearance (below detection limit) within one week after treatment initiation. Initiation of doxycycline treatment at the later time points resulted in clearance (below detection limit) of the infection from both lungs and spleens. By the end of the experiments, bacilli could no longer be cultured in the ∆metX-DUC (Fig. 6f) infected mice, and only ∆thrA-DUC infected mice that began doxycycline treatment at week 6 still showed detectable levels of bacteria (Fig. 6b). The total bacterial burden had been reduced by 4-logs in the lungs and >1-log in the spleens (Fig. 6d, h, respectively). Inspection of gross pathology and H&E staining of lungs harvested 189 days after infection (indicated by arrow P and dotted line in Fig. 6b, f) reveal typical tuberculous lesions in untreated mice with high bacterial burden and absence of lesions and inflammatory foci in mice that were switched to doxy chow (Fig. 6c, g). These experiments demonstrate the essentiality of the aspartate pathway in both acute and chronic Mtb infections in animals and show that Mtb is unable to scavenge nutrients from the host to complement these auxotrophies in vivo.
Significant efforts to identify new drug targets in Mtb have focused on the metabolism of essential nutrients. Mtb is an amino acid prototroph that has developed nominal machinery to obtain nutrients from the host, unlike many other intracellular parasites12,38 and consequently, Mtb appears to be particularly susceptible to inhibition of amino acid biosynthesis12. Moreover, the biosynthetic enzymes for essential amino acids are largely absent in humans and mammals, making amino acid biosynthetic pathways in Mtb attractive drug targets12,39,40,41,42.
To date, in vitro transposon sequencing (Tn-seq) screens have been used to predict gene essentiality in Mtb43,44 and have guided target selection in drug discovery. The usefulness of Tn-seq screens for the TB research field is undisputed, yet their limitations for drug discovery need consideration. A recent study highlighted the impact of growth medium on inferred gene essentiality45 and illustrated how in vitro Tn-seq screens can be limited predictors of in vivo essentiality and cannot differentiate between lethality, bacteriostasis, slow growth phenotypes or conditional essentiality, all information that is crucial for assessing druggability. Since M. tuberculosis is an intracellular pathogen, essentiality and druggability of targets have to be tested during chronic infection in order to prevent false targets being taken forward for drug development.
We here focused on the aspartate pathway, because it produces multiple essential building blocks for vital cellular functions in Mtb, such as cell wall biosynthesis, translation, and one-carbon metabolism. The rapid cell death phenotypes observed for auxotrophs of threonine (this study), homoserine (this study) and methionine13, points to a distinct susceptibility of Mtb to inhibition of this pathway. The mechanism of action for the lethality of threonine and homoserine auxotrophy appear to be multi-layered. Cell death kinetics due to the loss of proteinogenic amino acids is likely accelerated by the accumulation of intermediates of lysine biosynthesis and homoserine (only in thrB mutant).
By studying the metabolic response to aspartate pathway inhibition, we discovered that Mtb employs a combination of feedback control, overflow metabolism and catabolic action to prevent flux imbalances and ensure balanced precursor production. We show here corroborating evidence that the committed step of the aspartate pathway in Mtb, aspartate kinase, is controlled by allosteric feedback of threonine, but not by lysine or methionine. As Mtb lacks the ubiquitously used lysine-AK feedback loop, it must employ other regulatory mechanism to control production of proteinogenic lysine and the cell-wall building block diaminopimelate. By studying the adaptive metabolism of homoserine and threonine auxotrophic strains, we discovered two compensatory mechanisms that help Mtb to control the flux through this pathway branch: lysine degradation and export (Fig. 7b).
The lysine catabolic pathway catalyzed by Lat and Pcd is a unique feature of mycobacteria (Fig. 7). In a survey of 1362 bacteria, the aminoadipate branch was found to exist in only 36 microorganisms, predominately species of mycobacteria. This catabolic pathway seems to be a remnant of the cephamycin C biosynthetic pathway found in Streptomyces46, yet mycobacteria have only retained the first two reactions (mycobacteria do not produce cephamycin C). Another unique feature of this pathway in mycobacteria is the localization of lat in an operon with the alternative sigma factor sigF (Rv3286c) and lrp (Rv3291c)47 the putative transcriptional regulator of lat. SigF is important under various stress conditions, including osmotic stress, pH, heat-shock, oxidative stress48,49, and during infection50,51. Expression of lrp and lat genes is enriched in a persistence model17, as part of the stringent response16,18 and whenever Mtb transitions from replicating to non-replicating conditions (e.g., starvation or drug inhibition)16,17. These observations fit well with the increased abundance of lysine and aminoadipate observed in stationary phase cells (Supplementary Fig. 8). It is tempting to speculate that Mtb has lost lysine feedback control at the AK level in order to allow increased lysine flux to act as a signal for cellular stress. In this model, elevated intracellular lysine levels would cause upregulation of the Lat degradation pathway, which generates aminoadipate and leads to the activation of the stringent response and persistence. Alternatively, lysine catabolism and its potential toxic intermediate(s) may serve as a means to control growth under conditions where replication could be lethal, similar to the role of Toxin-Antitoxin modules52 or methylglyoxal metabolism in persister cell formation53. Potential candidates for toxic intermediates are aminoadipate semialdehyde and piperideine-6-carboxylate (Fig. 1a), as both have been shown to be cytotoxic54,55.
The second mechanism that mycobacteria employ to compensate for a missing lysine-AK feedback loop is catalyzed by a dedicated lysine/arginine permease LysE, encoded by Rv1986. We show that LysE in Mtb is used as a metabolic relief valve to clear excess cytoplasmic lysine, as a result of threonine auxotrophy. This exporter also has a role under non-auxotrophic conditions as evidenced by the retarded exit from lag phase and slow growth phenotype of the Mtb ∆lysE mutant. Current literature shows that Rv1986 is induced during infection of resting and activated macrophages56, as well as in a lysosomal exposure model57 and it plays a role during latent TB infection in humans58. The exporter is a dominant target of IL-2 secreting memory T cells and is proposed to contribute to protective immunity in humans58. In fact, amino acids, specifically arginine, were shown to modulate human immunometabolism and T-cell responses59. Together, these data suggest that LysE-mediated export of arginine, and possibly lysine, might play a role in shaping Mtb’s niche during infection.
Our current knowledge of the nutritional composition of the Mtb microenvironment in the host is still incomplete. How that environment evolves over the course of an infection is even less understood6,13,35. Auxotrophic bacterial strains are essential tools for identifying metabolic drug targets required during infection and probing the host environment for specific metabolites. However, because most Mtb auxotrophs fail to establish infection, their requirement for late-stage persistence cannot be investigated. To date, no data is available on the vulnerability of amino acid biosynthetic pathways during Mtb persistence in vivo. By utilizing conditional knockdowns of two branch-point enzymes (metX and thrA), we uncovered the aspartate pathway as being broadly required for persistent infection in mice. These data also clearly demonstrate the inability of Mtb to scavenge sufficient methionine, homoserine or threonine from the host throughout the course of infection. The observations presented here lay an important foundation for future drug development. We propose that the numerous essential enzymes identified in this pathway and their absence in eukaryotic cells make it particularly amenable to drug discovery efforts.
Mycobacterial strain and growth conditions
All strains and plasmids used in this study are listed in Supplementary Tables 1. Mycobacterial strains were grown in Middlebrook 7H9 medium (Difco) supplemented with 10% (vol/vol) OADC enrichment (0.5 g oleic acid, 50 g albumin, 20 g dextrose, 0.04 g catalase, 8.5 g sodium chloride in 1 L water), 0.2% (vol/vol) glycerol, and 0.05% (vol/vol) tylaxopol (Sigma). Antibiotic selection media contained 75 µg/mL hygromycin B, 20 µg/mL Kanamycin, and/or 25 µg/mL streptomycin, as required. Supplemented media for culturing auxotrophic mutants contained 50 µg/mL methionine, 500 µg/mL threonine, and/or 50 µg/mL homoserine. For time-course starvation and supplement growth curve experiments, strains were grown in the presence of the required supplements to an OD600 of 0.5, washed three times with PBS + 0.05% tylaxopol, and diluted into supplement free medium to an OD600 of 0.01 (growth/kill curves) or 0.2 (metabolomics and transcriptomics). Samples from three independent biological replicates were harvested on days 0, 2, 4 and 7 (∆thrA) or days 0, 1, 2 (∆thrB) for RNA extractions, and days 0, 1 and 2 for metabolite extractions (see below). Chronologically we studied the ∆thrA strain first and noticed that the main transcriptomic and metabolic changes are happening in the first 2 days. Hence, we focused on this timeframe for the rest of the study. Anhydrotetracycline (Acros) was dissolved in DMSO and used at the specified concentrations.
Gene Knockout and complementation
The genes thrA (Rv1294), thrB (Rv1296), lysE (Rv1986), and lysG (Rv1985c) were deleted in Mtb H37Rv by specialized transduction60. The Mtb H37Rv ∆metX strain (previously known as ∆metA) was constructed previously13. Transductants were recovered on selective medium containing hygromycin (75 μg/mL) and appropriate amounts of supplements when needed: homoserine (50 μg/mL) for Mtb ∆thrA and threonine (500 μg/mL) for Mtb ∆thrB. Mutations were confirmed by three-primer PCR using respective L, R, and Universal_uptag primers, listed in Supplementary Table 2. The H37Rv ∆metX and ∆thrA strains were complemented using the tetracycline-inducible dual-control (DUC) knockdown plasmids61. Briefly, each strain was complemented with pGMCK-q19-T38S38-P750-yfg-DAS+4 (pGMCK-yfg). The gene sequences were PCR-amplified using the respective P1 and P2 primers (Supplementary Table 2) and were recombined into pDO12A using BP clonase (Invitrogen), to generate the entry vectors pEN12A-yfg-DAS+4. The final construct was generated by 3-way gateway cloning with pEN23A-yfg-DAS + 4, pEN41A-T38S38, pEN12A-P750, and pDE43-MCK using LR clonase II (Invitrogen), to generate the final construct. This was transformed into the respective mutant strain to generate DAS complements whose expression of the complemented genes was under a TetOFF promoter. The H37Rv metX-DAS and thrA-DAS strains were further transformed with pGMCtKq28-TSC10M1-sspB to introduce Tet-inducible degradation of DAS+4 tagged proteins. Shine-delgarno sequences were mutated according to Supplementary Table 3, using Phusion Site-directed Mutagenesis kits (NEB). The H37Rv ∆lysE strain was complemented by transformation with pMV361 harboring a copy of Rv1986 (Supplementary Table 2). This DNA fragment was PCR amplified using primers Rv1986_fw_EcoR1 and Rv1986_Re_HindIII (Supplementary Table 2) and was cloned into pMV361 using EcoRI and HindIII restriction sites, resulting in plasmid pMV361-LysE.
Samples of bacterial cultures in biological triplicates were harvested at given time points13,62. For intracellular metabolites, an equivalent of 10 mL culture at an OD600 of 0.2 was rapidly filtered on a 0.22 µm nitrocellulose filter (Millipore). The filter papers were immediately placed in 2-mL screw cap tubes of 1 mL extraction solvent containing 20%/40%/40% (vol/vol) water/acetonitrile/methanol (Fisher) with approximately 500 µL of silica beads at −20 °C. The samples were homogenized twice in a Precellys Evolution (Bertin) at 4,500 rpm for 45 seconds, cooled to 5 °C using a Cryolys (Bertin), and with 5 min rest between cycles. Samples were centrifuged, and 750 µL of the extract was filtered through 0.22-µm Spin-X centrifuge filters (Corning, Life Technologies) at 10,621 g for 3 min, and stored at −80 °C. For extracellular metabolites, 1 mL of culture was collected and centrifuged, and 750 µL of supernatant was filtered twice through 0.22-µm Spin-X columns. Detergent in the samples were removed using Pierce detergent removal spin columns (Thermo), according to manufacturer’s instructions. Metabolites were extracted by adding 200 µL sample to 800 µL of 50%/50% (vol/vol) acetonitrile/methanol (Fisher), the samples were spun down, as before, and the supernatant collected and stored at −80 °C until analysis.
Metabolomics analysis was performed using an Acquity UPLC system coupled with a Synapt G2 quadrupole–time of flight hybrid mass spectrometer (Waters, Massachusetts, USA)13. Column eluents were delivered via electrospray ionization. UPLC was performed in a hydrophilic interaction liquid chromatography-mode (HILIC) gradient elution using an Acquity 1.7-μm amide column (2.1 × 100 mm)63. The flow rate is 0.5 mL/min with mobile phase A (100% acetonitrile) and mobile phase B (100% water), both containing 0.1% formic acid. In both positive and negative mode, the gradient began with 1% B until 1 min, ramped to 35% B by 14 min, then 60% B by 17 min, held at 60% B for 1 min, then ramped to 1% B by 19 min and held at 1% B to the end of run at 20 min. The mass spectrometer was operated in V mode for high sensitivity using a capillary voltage of 2 kV and a cone voltage of 17 V. The desolvation gas flow rate was 500 L/h, and the source and desolvation gas temperature were 120 °C and 325 °C, respectively. MS spectra were acquired in centroid mode from m/z 50–1,200 with a scan time of 0.5 s. Leucine enkephalin (2 ng/μL) was used as lock mass (m/z 556.2771 and 554.2615 in positive and negative experiments, respectively). Analysis was performed using MarkerLynx (Waters) with extended statistic function to identify statistically significant differences of metabolite abundances. A TargetLynx (Waters) database was compiled by running standards of metabolites of interest to determine retention times and m/z ratios. Calibration curves of compound mixes are run routinely to determine the linear range of metabolite detection. All samples were analyzed using TargetLynx with manual curation of peak areas where necessary. With abundances we refer to are raw intensity values for the area under the curve for each metabolite peak. Peak areas were used to calculate fold changes of metabolites relative to day 0. Metabolite abundances, retention times and m/z values can be found in Supplementary Data 1. Threonine and homoserine have the same molecular mass. The retention time of homoserine is 0.1–0.2 min slower than threonine, however differentiation of the two peaks is difficult. Fragmentation pattern of the two compounds in positive mode is nearly identical while in negative mode there is one distinction (m/z 72.04). We have detected high amounts of m/z = 120.0655 in the ThrB strain but not in Rv or ThrA. Since ThrB is downstream of homoserine, we hypothesize that this mass must represent homoserine, because the bacterium does not grow without the addition of high concentration threonine. In the ThrA strain, as expected from a strain that cannot produce homoserine nor threonine, the m/z 120.0655 was undetectable.
Samples of bacterial cultures were harvested in triplicate at appropriate times. 10 mL of culture was pelleted and the supernatant decanted. The cell pellet was resuspended in 1 mL of TRIzol (Invitrogen) and incubated overnight at 4 °C, before storage at −80 °C. The suspension was transferred to Fast-Prep Blue Cap tubes and processed twice for 45 s at speed 6 in a Fast-Prep apparatus (MP Biomedicals). After a brief incubation on ice, the debris was spun down, and the supernatant (750 μL) was processed for purification (described below).
Microarray (Mtb ∆thrA)
Total RNA was purified from the cell lysate using Direct-zol RNA MiniPrep (Zymo Research) with on-column DNase I according to the manufacturer’s protocol. Total RNA (2 μg) was used to create cDNA labeled with aminoallyl dUTP (Sigma). Fluorescent Cy3 and Cy5 dyes (GE Healthcare) then were covalently attached to the aminoallyl tags. Each pair of differentially labeled probes was resuspended in 60 μL of hybridization buffer (500 μL formamide, 250 μL 20 × SSC, 5 μL 10% (wt/vol) SDS, 245 μL ultrapure water) and hybridized to the microarray slide overnight in a 42 °C water bath. Slides then were washed in increasingly stringent wash conditions (three times for 5 min each washing in 1 × SSC 0.1% SDS; three times 5 min each washing in 0.1 × SSC 0.1% SDS; three times for 5 min each washing in 0.1 × SSC, and a final dip in 0.22-μm–filtered Milli-Q water [Millipore]). Arrays were scanned in a Genepix 4000A scanner, and spots were quantified with TIGR Spotfinder. The data then were processed in TIGR MIDAS. Two-color tiff images of the microarrays were inspected visually for defects and obvious spatial biases. Before normalization, pin-tip (block) intensity box plots were used to detect slides exhibiting spatial and/or pin biases; after normalization, intensity box plots and MA plots were used to assess the effectiveness of normalization in correcting these biases. Radio-intensity plots were used to identify outlier slides and to assess the effectiveness of the normalization process, and Z-score histograms were used to look for slides with abnormal intensity distributions. Slides that did not pass the quality-control process were rejected, and repeat hybridizations were performed. After normalization (total intensity and LOWESS) the in-slide replicate spots were averaged before expression ratios were calculated. The results from four independent biological replicates including two dye swaps then were subjected to a t-test without false discovery correction in TIGR MeV software. The analysis was used as a ranking method. For a general overview, genes with expression ratios >2 and <0.5 and a P-value <0.05 were used for data interpretation.
RNA-seq (Mtb ∆thrB)
RNA from the clarified cell lysate samples were purified by Trizol®-chlorofom precipitation according to the manufacturer instructions (Invitrogen). After purification remaining DNA was removed from the samples using the DNA-Free Turbo DNase Kit (Ambion) and RNA integrity was checked on a Bioanalyzer RNA 6000 Pico chip (Agilent). The ribosomal RNA (rRNA) was removed using the Bacterial RiboZero kit (Illumina), and removal was confirmed by Bioanaylzer as above. RNA-seq library preparation was conducted with the TrueSeq Stranded mRNA Library Prep (Illumina) according to manufacturer’s instructions and the library was sequenced on a NextSeq 500 (Illumina) using the NextSeq 500/550 HO V2 (75 cycles) (Illumina). Illumina reads were mapped to the M. tuberculosis reference genome from NCBI (NC_000962.3) in the form of a SAM file using Bowtie2 (http://bowtie-bio.sourceforge.net/index.shtml), the SAM files were converted to coordinate-sorted BAM files using samtools, and reads over genes were counted using featureCounts64. Differential expression analysis was then conducted using R and the DESeq2 package.
Mouse studies were performed in accordance with National Institutes of Health guidelines following the recommendations in the Guide for the Care and Use of Laboratory Animals65. The protocols used in this study were approved by the Institutional Animal Care and Use Committee of Albert Einstein College of Medicine (Protocols #20120114 and #20180612).
Female SCID mice and female C57BL/6 mice (Jackson Laboratories) were infected via the aerosol route using a 1 × 107 cfu/mL mycobacterial suspension in PBS containing 0.05% tylaxopol and 0.004% antifoam. Infection yielded approximately 100 bacilli per lung as determined by quantification of lung bacterial loads at 24 h post-infection (four mice per group). Subsequently, four mice from each group were killed at days 1, 7, 21, 63, 84, 98 (C57BL/6) or 1, 14, 22, and 42 (SCID) to determine the bacterial burden in the lung and spleen. Six SCID mice per group were kept for survival experiments. For conditional knockdown experiments, groups of mice infected with each strain were started on 2000 ppm doxycycline-treated chow (TestDiet, Missouri, USA) at 0, 1, 3, and 6 weeks. Four mice from each group were sacrificed at given times, the lungs and spleens were harvested, homogenized and plated on 7H10 media containing the appropriate supplement to determine the bacterial burden. All mice infected with Mtb were maintained under appropriate conditions in an animal biosafety level 3 laboratory.
Lung samples were fixed in 10% neutral buffered formalin for 48–72 h and the subjected to paraffin embedment. Tissues were sectioned at 5 µm and stained with Hematoxylin and Eosin (H&E).
MIC determination of toxic metabolite analogs
Cultures of Mtb H37Rv, ∆lysE, ∆lysEcomp, and ∆lysG were grown to log-phase in unsupplemented media. Each toxic analog (Supplementary Fig. 1) was two-fold serially diluted in a sterile 96 well plate. In triplicate, each strain was diluted to an OD600 of 0.001 in wells containing each of the drugs to a final volume of 0.2 mL. The plates were incubated at 37 °C for 7 days and the growth was measured by optical density in an Epoch plate reader (Biotek, Vermont, USA). Percent growth was calculated based on the density in the untreated wells. For arginine rescue experiments, arginine was added to each well at a concentration of 50 µg/ml.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
WHO. Global Tuberculosis Report 2017. (Geneva, Switzerland, 2017).
Dartois, V. The path of anti-tuberculosis drugs: from blood to lesions to mycobacterial cells. Nat. Rev. Microbiol 12, 159–167 (2014).
Connolly, L. E., Edelstein, P. H. & Ramakrishnan, L. Why is long-term therapy required to cure tuberculosis? PLoS Med. 4, e120 (2007).
Rhee, K. Y. et al. Central carbon metabolism in Mycobacterium tuberculosis: an unexpected frontier. Trends Microbiol 19, 307–314 (2011).
Ehrt, S., Schnappinger, D. & Rhee, K. Y. Metabolic principles of persistence and pathogenicity in Mycobacterium tuberculosis. Nat. Rev. Microbiol 16, 496–507 (2018).
Warner, D. F. Mycobacterium tuberculosis metabolism. Cold Spring Harb. Perspect. Med. 5, pii: a021121 (2014).
Ruecker, N. et al. Fumarase deficiency causes protein and metabolite succination and intoxicates Mycobacterium tuberculosis. Cell Chem. Biol. 24, 306–315 (2017).
Trujillo, C. et al. Triosephosphate isomerase is dispensable in vitro yet essential for Mycobacterium tuberculosis to establish infection. MBio 5, e00085 (2014).
Puckett, S. et al. Inactivation of fructose-1,6-bisphosphate aldolase prevents optimal co-catabolism of glycolytic and gluconeogenic carbon substrates in Mycobacterium tuberculosis. PLoS Pathog. 10, e1004144 (2014).
Puckett, S. et al. Glyoxylate detoxification is an essential function of malate synthase required for carbon assimilation in Mycobacterium tuberculosis. Proc. Natl. Acad. Sci. USA 114, E2225–E2232 (2017).
Eoh, H. et al. Metabolic anticipation in Mycobacterium tuberculosis. Nat. Microbiol 2, 17084 (2017).
Berney, M. & Berney-Meyer, L. Mycobacterium tuberculosis in the Face of Host-Imposed Nutrient Limitation. Microbiol Spectr. 5, TBTB2-0030-2016 (2017).
Berney, M. et al. Essential roles of methionine and S-adenosylmethionine in the autarkic lifestyle of Mycobacterium tuberculosis. Proc. Natl Acad. Sci. USA 112, 10008–10013 (2015).
Pavelka, M. S. Jr. & Jacobs, W. R. Jr. Biosynthesis of diaminopimelate, the precursor of lysine and a component of peptidoglycan, is an essential function of Mycobacterium smegmatis. J. Bacteriol. 178, 6496–6507 (1996).
Viola, R. E. The central enzymes of the aspartate family of amino acid biosynthesis. Acc. Chem. Res. 34, 339–349 (2001).
Betts, J. C., Lukey, P. T., Robb, L. C., McAdam, R. A. & Duncan, K. Evaluation of a nutrient starvation model of Mycobacterium tuberculosis persistence by gene and protein expression profiling. Mol. Microbiol 43, 717–731 (2002).
Keren, I., Minami, S., Rubin, E. & Lewis, K. Characterization and transcriptome analysis of Mycobacterium tuberculosis persisters. MBio 2, e00100–e00111 (2011).
Duan, X. et al. Mycobacterium Lysine epsilon-aminotransferase is a novel alarmone metabolism related persister gene via dysregulating the intracellular amino acid level. Sci. Rep. 6, 19695 (2016).
Schneefeld, M., Busche, T., Geffers, R., Kalinowski, J. & Bange, F. C. The transcriptional regulator LysG (Rv1985c) of Mycobacterium tuberculosis activates lysE (Rv1986) in a lysine-dependent manner. PLoS ONE 12, e0186505 (2017).
O’Barr, T. P. & Everett, K. A. Effect of l-homoserine on the growth of Mycobacterium tuberculosis. Infect. Immun. 3, 328–332 (1971).
Stadtman, E. R. Symptosium on multiple forms of enzymes and control mechanisms. II. Enzyme multiplicity and function in the regulation of divergent metabolic pathways. Bacteriol. Rev. 27, 170–181 (1963).
Cremer, J., Treptow, C., Eggeling, L. & Sahm, H. Regulation of enzymes of lysine biosynthesis in Corynebacterium glutamicum. J. Gen. Microbiol 134, 3221–3229 (1988).
Atkinson, D. E. Regulation of enzyme function. Annu Rev. Microbiol 23, 47–68 (1969).
Patte, J. C., Le Bras, G. & Cohen, G. N. Regulation by methionine of the synthesis of a third aspartokinase and of a second homoserine dehydrogenase in Escherichia coli K 12. Biochim Biophys. Acta 136, 245–247 (1967).
Nakayama, K., Kitada, S. & Kinoshita, S. Studies on lysine fermentation I. The control mechanism on lysine accumulation by homoserine and threonine. J. Gen. Appl. Microbiol. 7, 145–154 (1961).
Nakayama, K., Tanaka, H., Hagino, H. & Kinoshita, S. Studies on lysine fermentation Part V. Concerted feedback inhibition of aspartokinase and the absence of lysine inhibition on aspartic semialdehyde-pyruvate condensation in micrococcus glutamicus. Agric. Biol. Chem. 30, 611–616 (1966).
Yang, Q. et al. Structural view of the regulatory subunit of aspartate kinase from Mycobacterium tuberculosis. Protein Cell 2, 745–754 (2011).
Weinberg, Z. et al. The aptamer core of SAM-IV riboswitches mimics the ligand-binding site of SAM-I riboswitches. RNA 14, 822–828 (2008).
Bellmann, A. et al. Expression control and specificity of the basic amino acid exporter LysE of Corynebacterium glutamicum. Microbiology 147, 1765–1774 (2001).
Erdmann, A., Weil, B. & Kramer, R. Lysine secretion by wild-type Corynebacterium glutamicum triggered by dipeptide uptake. J. Gen. Microbiol 139, 3115–3122 (1993).
Nandineni, M. R. & Gowrishankar, J. Evidence for an arginine exporter encoded by yggA (argO) that is regulated by the LysR-type transcriptional regulator ArgP in Escherichia coli. J. Bacteriol. 186, 3539–3546 (2004).
Cai, T. et al. Host legume-exuded antimetabolites optimize the symbiotic rhizosphere. Mol. Microbiol 73, 507–517 (2009).
Davis, A. L., Lloyd, R., Maul, S., Cook, D. E. & McCord, T. J. 2,6-Diamino-4-hexynoic acid, a lysine analog. Arch. Biochem Biophys. 104, 238–240 (1964).
Kulis-Horn, R. K., Persicke, M. & Kalinowski, J. Corynebacterium glutamicum ATP-phosphoribosyl transferases suitable for L-histidine production-strategies for the elimination of feedback inhibition. J. Biotechnol. 206, 26–37 (2015).
Kim, J. H. et al. A genetic strategy to identify targets for the development of drugs that prevent bacterial persistence. Proc. Natl Acad. Sci. USA 110, 19095–19100 (2013).
Woong Park, S. et al. Evaluating the sensitivity of Mycobacterium tuberculosis to biotin deprivation using regulated gene expression. PLoS Pathog. 7, e1002264 (2011).
Wei, J. R. et al. Depletion of antibiotic targets has widely varying effects on growth. Proc. Natl Acad. Sci. USA 108, 4176–4181 (2011).
Zhang, Y. J. & Rubin, E. J. Feast or famine: the host-pathogen battle over amino acids. Cell. Microbiol. 15, 1079–1087 (2013).
Evans, J. C. & Mizrahi, V. The application of tetracyclineregulated gene expression systems in the validation of novel drug targets in Mycobacterium tuberculosis. Front Microbiol 6, 812 (2015).
Wellington, S. et al. A small-molecule allosteric inhibitor of Mycobacterium tuberculosis tryptophan synthase. Nat. Chem. Biol. 13, 943–950 (2017).
Zhang, Y. J. et al. Tryptophan biosynthesis protects mycobacteria from CD4 T-cell-mediated killing. Cell 155, 1296–1308 (2013).
Wellington, S. & Hung, D. T. The Expanding Diversity of Mycobacterium tuberculosis Drug Targets. ACS Infect. Dis. 4, 696–714 (2018).
DeJesus, M. A., et al. Comprehensive essentiality analysis of the Mycobacterium tuberculosis Genome via saturating transposon mutagenesis. MBio 8, pii: e02133-16 (2017).
Sassetti, C. M., Boyd, D. H. & Rubin, E. J. Genes required for mycobacterial growth defined by high density mutagenesis. Mol. Microbiol 48, 77–84 (2003).
Minato, Y., et al. Genomewide assessment of Mycobacterium tuberculosis conditionally essential metabolic pathways. mSystems 4, pii: e00070-19 (2019).
Liras, P. Biosynthesis and molecular genetics of cephamycins. Cephamycins produced by actinomycetes. Antonie Van. Leeuwenhoek 75, 109–124 (1999).
Neshich, I. A., Kiyota, E. & Arruda, P. Genome-wide analysis of lysine catabolism in bacteria reveals new connections with osmotic stress resistance. ISME J. 7, 2400–2410 (2013).
Gebhard, S., Humpel, A., McLellan, A. D. & Cook, G. M. The alternative sigma factor SigF of Mycobacterium smegmatis is required for survival of heat shock, acidic pH and oxidative stress. Microbiology 154, 2786–2795 (2008).
Humpel, A., Gebhard, S., Cook, G. M. & Berney, M. The SigF regulon in Mycobacterium smegmatis reveals roles in adaptation to stationary phase, heat and oxidative stress. J. Bacteriol. 192, 2491–2502 (2010).
Chen, P., Ruiz, R. E., Li, Q., Silver, R. F. & Bishai, W. R. Construction and characterization of a Mycobacterium tuberculosis mutant lacking the alternate sigma factor gene, sigF. Infect. Immun. 68, 5575–5580 (2000).
Karls, R. K., Guarner, J., McMurray, D. N., Birkness, K. A. & Quinn, F. D. Examination of Mycobacterium tuberculosis sigma factor mutants using low-dose aerosol infection of guinea pigs suggests a role for SigC in pathogenesis. Microbiology 152, 1591–1600 (2006).
Sala, A, Bordes, P. & Genevaux, P. Multiple toxin-antitoxin systems in Mycobacterium tuberculosis. Toxins (Basel). 6, 1002–1020 (2014).
Girgis, H. S., Harris, K. & Tavazoie, S. Large mutational target size for rapid emergence of bacterial persistence. Proc. Natl Acad. Sci. USA 109, 12740–12745 (2012).
Zaret, K. S. & Sherman, F. alpha-Aminoadipate as a primary nitrogen source for Saccharomyces cerevisiae mutants. J. Bacteriol. 162, 579–583 (1985).
Mills, P. B. et al. Mutations in antiquitin in individuals with pyridoxine-dependent seizures. Nat. Med. 12, 307–309 (2006).
Schnappinger, D. et al. Transcriptional adaptation of Mycobacterium tuberculosis within macrophages: insights into the phagosomal environment. J. Exp. Med. 198, 693–704 (2003).
Lin, W. et al. Transcriptional profiling of Mycobacterium tuberculosis exposed to in vitro lysosomal stress. Infect. Immun. 84, 2505–2523 (2016).
Gideon, H. P. et al. Hypoxia induces an immunodominant target of tuberculosis specific T cells absent from common BCG vaccines. PLoS Pathog. 6, e1001237 (2010).
Geiger, R. et al. L-Arginine modulates T cell metabolism and enhances survival and anti-tumor activity. Cell 167, 829–842 e813 (2016).
Jain, P. et al. Specialized transduction designed for precise high-throughput unmarked deletions in Mycobacterium tuberculosis. MBio 5, e01245–01214 (2014).
Schnappinger, D., O’Brien, K. M. & Ehrt, S. Construction of conditional knockdown mutants in mycobacteria. Methods Mol. Biol. 1285, 151–175 (2015).
Noy, T. et al. Central role of pyruvate kinase in carbon co-catabolism of Mycobacterium tuberculosis. J. Biol. Chem. 291, 7060–7069 (2016).
Paglia, G. et al. Monitoring metabolites consumption and secretion in cultured cells using ultra-performance liquid chromatography quadrupole-time of flight mass spectrometry (UPLC-Q-ToF-MS). Anal. Bioanal. Chem. 402, 1183–1198 (2012).
Benjak, A., Sala, C. & Hartkoorn, R. C. Whole-transcriptome sequencing for high-resolution transcriptomic analysis in Mycobacterium tuberculosis. Methods Mol. Biol. 1285, 17–30 (2015).
Council, N. R. Guide for the Care and Use of Laboratory Animals: Eighth Edition, (The National Academies Press, Washington, DC, 2011).
This study was financially supported by NIH funding AI119573 and AI139465 for M.B., D.R.S., and E.H. and T32-GM007288 and AI138483 for E.H. S.J. was supported by NIH grant T32 AI007501. G.C. was supported by Marsden Fund NZ. J.M.T. was supported by effect:hope (Leprosy Mission Canada) on behalf of the Research to Stop Neglected Tropical Disease Transmission (R2STOP) Initiative. W.R.J. was supported by AI026170. We thank Dirk Schnappinger for providing the plasmids for making the DUC constructs and Sabine Ehrt for helping out with doxy chow. We thank John Kim, Mei Chen, Annie Zhi Dai, Bing Chen, Robert Dubin, Xusheng Zhang, and Fabien Delahaye for technical support and Kevin Pethe for critical reading of the manuscript.
The authors declare no competing interests.
Peer review information Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work. Peer reviewer reports are available.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Hasenoehrl, E.J., Rae Sajorda, D., Berney-Meyer, L. et al. Derailing the aspartate pathway of Mycobacterium tuberculosis to eradicate persistent infection. Nat Commun 10, 4215 (2019). https://doi.org/10.1038/s41467-019-12224-3
Structural analysis of mycobacterial homoserine transacetylases central to methionine biosynthesis reveals druggable active site
Scientific Reports (2019)