Mycobacterium tuberculosis (Mtb) infection is notoriously difficult to treat. Treatment efficacy is limited by Mtb’s intrinsic drug resistance, as well as its ability to evolve acquired resistance to all antituberculars in clinical use. A deeper understanding of the bacterial pathways that influence drug efficacy could facilitate the development of more effective therapies, identify new mechanisms of acquired resistance, and reveal overlooked therapeutic opportunities. Here we developed a CRISPR interference chemical-genetics platform to titrate the expression of Mtb genes and quantify bacterial fitness in the presence of different drugs. We discovered diverse mechanisms of intrinsic drug resistance, unveiling hundreds of potential targets for synergistic drug combinations. Combining chemical genetics with comparative genomics of Mtb clinical isolates, we further identified several previously unknown mechanisms of acquired drug resistance, one of which is associated with a multidrug-resistant tuberculosis outbreak in South America. Lastly, we found that the intrinsic resistance factor whiB7 was inactivated in an entire Mtb sublineage endemic to Southeast Asia, presenting an opportunity to potentially repurpose the macrolide antibiotic clarithromycin to treat tuberculosis. This chemical-genetic map provides a rich resource to understand drug efficacy in Mtb and guide future tuberculosis drug development and treatment.
Infections caused by the bacterial pathogen Mycobacterium tuberculosis (Mtb) are notoriously difficult to treat. While the reasons necessitating prolonged chemotherapy are multifactorial1,2, the intrinsic resistance of Mtb and its ability to evolve acquired resistance to all antituberculars in clinical use are major barriers to successful treatment3,4.
While comparatively underexplored, intrinsic resistance in Mtb is typically ascribed to the low permeability of the cell envelope and the numerous efflux pumps encoded in the Mtb genome5,6,7. Acquired drug resistance in Mtb occurs via mutation and many resistance mutations have been characterized in recent decades8. These mutations most commonly occur in the drug target or drug activator8,9,10. Yet, our knowledge of acquired drug resistance in Mtb remains incomplete, particularly for mutations outside of the drug target or activator and which typically confer low-to-intermediate, but clinically relevant, levels of drug resistance4,11,12.
To provide a genome-wide overview of the bacterial pathways that influence drug potency, we developed a CRISPR (Clustered Regularly Interspaced Short Palindromic Repeats) interference (CRISPRi)13,14,15,16,17 chemical-genetics platform to titrate the expression of nearly all Mtb genes (essential and non-essential) and quantify bacterial fitness in the presence of different drugs. This approach identified hundreds of genes whose inhibition altered fitness during drug treatment. Mining this dataset, we discovered diverse mechanisms of intrinsic drug resistance that can be targeted to potentiate therapy. Overlaying the chemical-genetic results with comparative genomics of Mtb clinical isolates, we identified previously unknown, clinically relevant mechanisms of acquired drug resistance. Lastly, we make the unexpected discovery of ‘acquired drug sensitivities’, whereby loss-of-function mutations in intrinsic drug resistance genes render some Mtb clinical strains hypersusceptible to clarithromycin, an antibiotic not typically used to treat tuberculosis (TB).
Defining genetic determinants of drug potency with CRISPRi
To define genes that influence drug potency in Mtb, we performed 90 CRISPRi screens across nine drugs in H37Rv Mtb. These screens used a genome-scale CRISPRi library15 to enable titratable knockdown for nearly all Mtb genes, including protein coding genes and non-coding RNAs (Fig. 1a). Knockdown tuning enabled hypomorphic silencing of in vitro essential genes15, thereby allowing quantification of chemical-genetic interactions for both essential and non-essential genes to provide a global overview of gene–drug interactions in Mtb.
Drugs were chosen to represent clinically relevant antituberculars as well as two drugs not traditionally used to treat TB (Supplementary Table 1). Drugs were screened at concentrations spanning the predicted minimum inhibitory concentration (MIC). After library outgrowth, we collected genomic DNA from cultures treated with three descending doses of partially inhibitory drug concentrations (Extended Data Fig. 1) and analysed sgRNA (single guide RNA) abundance by deep sequencing. Hit genes were identified by MAGeCK18. In total, we identified 1,373 genes whose knockdown led to sensitization and 775 genes whose knockdown led to resistance to at least one drug (Source Data Fig. 1). Most hit genes had a single chemical-genetic interaction, but some had as many as seven (Extended Data Fig. 2a).
The chemical-genetic screens recovered expected hit genes including direct drug targets, genes encoding the targets of known synergistic drug combinations and genes whose inactivation is known to confer acquired drug resistance (Fig. 1b–d)3,8,9,10,19. Benchmarking our CRISPRi approach against published transposon sequencing (TnSeq) chemical-genetic results revealed strong overlap (63.3–87.7% TnSeq hit recovery; Source Data Extended Data Fig. 3)3, although TnSeq as currently implemented in Mtb is restricted to interrogation of non-essential genes. The number of hit genes varied widely across drugs (Fig. 1e,f and Extended Data Fig. 2b–j). Interestingly, essential genes were enriched relative to non-essential genes for chemical-genetic interactions (Fig. 1e,f and Extended Data Fig. 3a), even when taking into account the bias towards sgRNAs targeting essential genes in the CRISPRi library. This enrichment demonstrates the increased information content available when assaying essential genes by chemical genetics. Hierarchical clustering revealed unique chemical-genetic signatures for each drug (Extended Data Fig. 3b), which were then mined for biological insight.
Although they target distinct cellular processes, clustering analysis revealed correlated chemical-genetic signatures for rifampicin (RIF), vancomycin (VAN) and bedaquiline (BDQ), suggesting shared mechanisms of intrinsic resistance or sensitivity. Enrichment analysis identified the essential mycolic acid-arabinogalactan-peptidoglycan (mAGP) complex to be a common sensitizing hit for these drugs, but not the ribosome-targeting drugs clarithromycin (CLR), linezolid (LZD) or streptomycin (STR) (Extended Data Fig. 3c). The mAGP is the primary constituent of the Mtb cell envelope and has long been known to serve as a permeability barrier that mediates intrinsic drug resistance6,7,20,21. Interestingly, it was not obvious which drug physiochemical properties were driving selective mAGP sensitization (Extended Data Fig. 3d)22. For example, despite similar molecular weights, bedaquiline displayed a strong mAGP signature, whereas streptomycin did not; despite similar polar surface areas, rifampicin displayed a strong mAGP signature, but clarithromycin did not.
To ensure the validity of the screen results, we quantified drug susceptibility with individual hypomorphic CRISPRi strains targeting mAGP-biosynthetic genes, demonstrating 2- to 43-fold reductions in IC50 (concentration required for 50% growth inhibition) for rifampicin, vancomycin and bedaquiline, but little to no change for linezolid (Extended Data Fig. 4a–d). To validate these results chemically, we focused on the β-ketoacyl-ACP synthase KasA, an enzyme essential for mycolic acid biosynthesis and an active drug target23,24. We confirmed that a small-molecule KasA inhibitor GSK3011724A (GSK’724A) synergizes with rifampicin, vancomycin and bedaquiline, but not linezolid, in laboratory culture and also confirmed GSK’724A-rifampicin synergy ex vivo in macrophages (Extended Data Fig. 4e–g). We found that Mtb pre-treated with GSK’724A showed increased uptake of ethidium bromide and a fluorescent vancomycin conjugate, suggesting that the drug synergies observed with GSK’724A may be explained, at least in part, by the ability of GSK’724A to disrupt mAGP integrity and promote drug uptake (Extended Data Fig. 4h,i). These results validate the screen and confirm the role of the mAGP complex as a selective mechanism of intrinsic resistance relevant for some antitubercular agents but not others25.
mtrA promotes envelope integrity and intrinsic resistance
Two of the most sensitizing hit genes across multiple drugs were mtrA and mtrB (Fig. 2a), which encode the response regulator MtrA and its cognate histidine kinase MtrB26,27. The mtrAB operon also encodes a putative lipoprotein lpqB (Fig. 2b). LpqB is proposed to interact with MtrB to promote MtrA phosphorylation and activation28. The similarities between the chemical-genetic signatures of mtrAB-lpqB and mAGP-biosynthetic genes (Fig. 2a and Extended Data Fig. 4b) suggest a role for this two-component system in regulating mAGP integrity. Given the predicted essentiality of mtrAB-lpqB26,29 and the magnitude by which their inhibition sensitized Mtb to antibiotics, we next sought to better define the mechanism by which mtrAB-lpqB promote intrinsic drug resistance.
Strong CRISPRi silencing of mtrA, mtrB and lpqB prevented Mtb growth (Fig. 2b). Inhibition of mtrA was bacteriostatic in laboratory culture but bactericidal in macrophages (Fig. 2c and Extended Data Fig. 5a,b). mtrA, mtrB and lpqB knockdown strongly sensitized Mtb to rifampicin, vancomycin and bedaquiline (Fig. 2d and Extended Data Fig. 5c). As with KasA inhibition (Extended Data Fig. 4h,i), silencing mtrA, mtrB, and to a lesser extent lpqB, led to increased permeability to ethidium bromide and a fluorescent vancomycin conjugate (Fig. 2e), suggesting that the increase in drug susceptibility with mtrAB-lpqB knockdown is at least in part mediated by increased envelope permeability.
To better understand the mechanism(s) by which mtrA promotes intrinsic resistance, we next defined its regulon. RNA-seq following mtrA silencing identified 41 downregulated and 11 upregulated genes (Fig. 2f and Source Data Fig. 2), many of which were previously found to bind MtrA by ChIP-seq (Extended Data Fig. 5d,e)27. We confirmed by quantitative reverse transcription PCR (RT-qPCR) that putative regulon genes activated by MtrA were downregulated following mtrAB knockdown (Extended Data Fig. 5f). Surprisingly, silencing lpqB produced the opposite result—MtrA regulon genes were upregulated (Extended Data Fig. 5g). In contrast to the proposed role of LpqB as a positive regulator of this pathway28, these data instead suggest that LpqB may negatively regulate MtrA signalling. To distinguish whether MtrA activation in the absence of LpqB is MtrB-dependent, we tested MtrA regulon expression upon simultaneous silencing of mtrB and lpqB. MtrA activation in the absence of LpqB required MtrB (Fig. 2g). Taken together, these results support a model whereby the extracytoplasmic lipoprotein LpqB functions as a negative regulator of MtrB to restrain MtrA activation.
The MtrA regulon encodes numerous peptidoglycan remodelling enzymes important for cell growth and division (Source Data Fig. 2)27,30,31. Intriguingly, several regulon genes were also identified as sensitizing hits in our screen, phenocopying the effects of mtrA silencing (Fig. 2a). mtrAB and regulon expression were not altered in response to drug treatment (Extended Data Fig. 5h). These results demonstrate the central role of the MtrAB signalling pathway in coordinating proper peptidoglycan remodelling during bacterial growth and division (Fig. 2h), and highlight the potential utility of small-molecule modulators of this pathway.
Diverse pathways influence potency of translation inhibitors
Inhibition of mAGP biosynthesis did not sensitize Mtb to the three ribosome-targeting drugs streptomycin, clarithromycin and linezolid (Extended Data Figs. 3c,d and 6a). Thus, mAGP inhibition is unlikely to be a relevant mechanism to potentiate activity of these drugs.
Streptomycin, clarithromycin and linezolid had correlated chemical-genetic signatures that appeared to be driven by the lack of a mAGP signature rather than any unique ribosome target signature (Extended Data Fig. 3b,c), which may reflect the different mechanisms of action of these drugs. Streptomycin interacts with the 30S ribosomal subunit and induces mis-translation32, whereas linezolid and clarithromycin both act on the 50S subunit to inhibit translation elongation33,34 (Fig. 3a). The sole sensitizing hit observed uniquely among the three ribosome-targeting drugs was whiB7, a transcription factor that induces a stress response promoting intrinsic resistance to numerous ribosome-targeting antibiotics35. The specific hit genes varied between these drugs but could be broadly classified into the following categories: ribosomal RNA (rRNA) methylation, drug efflux/import, ribosome rescue, ribosome regulation, proteasome activity and numerous poorly characterized genes (Fig. 3b,c).
Consistent with previous publications, we found that rRNA methyltransferases can confer either intrinsic sensitivity or intrinsic resistance to ribosome-targeting drugs36. For example, silencing erm(37) resulted in clarithromycin sensitivity (Fig. 3b)37, whereas silencing the 16S rRNA methyltransferase gid conferred streptomycin resistance38. Interestingly, knockdown of the predicted 23S rRNA methyltransferase tsnR conferred resistance to linezolid (Fig. 3b). This is analogous to work in Staphylococcus aureus, in which loss of the evolutionarily distinct 23S methyltransferase rlmN confers linezolid resistance both in vitro and in the clinic39. To determine whether loss-of-function tsnR mutations could play a clinically relevant role in acquired linezolid resistance, we assembled a database of >45,000 whole genome sequences from Mtb clinical isolates (Source Data Extended Data Fig. 8). Given the recent introduction of linezolid to TB treatment, we expected linezolid-resistant Mtb to be rare. Consistent with this, we identified the most common linezolid-resistance mutation rplC-Cys154Arg40 only 122 times in our genome database. While putative loss-of-function mutations in tsnR were even more rare (Source Data Fig. 3), two multidrug-resistant (MDR) Mtb strains harboured both a tsnR frameshift allele and an rplC-Cys154Arg allele, which are highly unlikely to have co-occurred by chance (χ2 test with Yates’ correction: P < 0.0001). These data highlight that loss-of-function tsnR mutations may serve as stepping stones to high-level resistance as linezolid is used more widely in the clinic.
We next sought to determine whether our findings could be exploited to identify synergistic drug–target combinations to overcome resistance and increase the therapeutic index for linezolid, analogous to preclinical efforts to boost ethionamide potency and tolerability41. The essential trans-translation genes, smpB and ssr29, were identified as linezolid-sensitizing hits (Fig. 3b,c). Trans-translation is a ribosome rescue pathway thought to primarily rescue ribosomes stalled on non-stop messenger RNAs42. Additionally, we identified the poorly characterized gene rv1473 as a linezolid-specific sensitizing hit (Fig. 3b,c). rv1473 was previously reported to be a macrolide efflux pump43. However, the lack of predicted transmembrane helices suggest that rv1473 is unlikely to be a membrane-embedded ABC transporter. Rather, homology suggests that rv1473 belongs to the family of antibiotic resistance ABC-F proteins, which have been shown to rescue drug-bound ribosomes by facilitating drug dissociation (Extended Data Fig. 6b)44,45.
Our data suggest that inhibition of rv1473 and trans-translation could make linezolid more potent. Individual CRISPRi knockdown of rv1473 and smpB lowered the IC50 for linezolid by 2.3- and 5-fold, respectively (Fig. 3d and Extended Data Fig. 6c). Inhibition of the Clp protease did not sensitize Mtb to linezolid (Extended Data Fig. 6d,e), consistent with the critical role of trans-translation in rescuing linezolid-stalled ribosomes, but not in Clp protease-mediated turnover of ssrA-tagged stalled translation products46. Dual CRISPRi knockdown of both rv1473 and smpB lowered the linezolid IC50 by 12.2-fold (Fig. 3d and Extended Data Fig. 6c), consistent with rv1473 and trans-translation functioning in separate intrinsic resistance pathways. Given the magnitude of linezolid sensitivity of the dual knockdown strain, we hypothesized that dual inhibition of rv1473 and smpB could functionally reverse linezolid resistance. Dual knockdown of rv1473 and smpB in a linezolid-resistant strain restored linezolid sensitivity back to wild-type (WT) levels (Fig. 3d and Extended Data Fig. 6f,g), demonstrating that inhibition of intrinsic resistance factors can potentiate linezolid and functionally reverse acquired drug resistance.
bacA mutations are a source of aminoglycoside resistance
Acquired drug resistance is a major barrier to successful TB treatment. However, our knowledge of the genetic basis of acquired drug resistance remains incomplete, particularly for mutations outside of the drug target or activator, and which typically confer low-to-intermediate, but clinically relevant, levels of drug resistance4,8,11,12. Given the ability of our chemical-genetic approach to identify hit genes associated with clinically relevant acquired drug resistance (Figs. 1b–d and 3b), we hypothesized that mining our chemical-genetic data may identify previously unrecognized mechanisms of acquired drug resistance in Mtb.
We chose to focus our search for sources of acquired drug resistance to streptomycin. Streptomycin has been used to treat TB since the late 1940s and thus Mtb has had decades of selective pressure to potentially give rise to a diverse set of resistance mutations. Aminoglycosides such as streptomycin must traverse the Mtb envelope to access their ribosomal target. The mechanism(s) of aminoglycoside uptake by Mtb are not well understood. Interestingly, and consistent with previous work47, the strongest streptomycin-resistance hit gene in our screen was bacA (rv1819c; Fig. 3b,c). Recently, structural and biochemical work demonstrated that bacA is an ABC importer of diverse hydrophilic solutes48. Thus, we hypothesized that bacA may serve as a streptomycin importer and that bacA loss-of-function mutants may be an unrecognized source of streptomycin resistance in clinical Mtb strains.
Searching our clinical strain genome database, we observed numerous bacA non-synonymous single nucleotide polymorphisms (SNPs) and small insertion-deletions (indels), and selected six for experimental validation (Fig. 4a and Source Data Fig. 4). Consistent with our hypothesis, four of the six bacA mutant strains displayed an elevated streptomycin MIC (Fig. 4b). Interestingly, these strains also showed elevated MICs to other aminoglycosides (amikacin and kanamycin) as well as the tuberactinomycin capreomycin (Extended Data Fig. 7a). Moreover, overexpression of Mtb bacA sensitized M. smegmatis to streptomycin (Extended Data Fig. 7b). While further studies are necessary to definitively show that bacA is an importer of aminoglycosides and tuberactinomycins, our data, in combination with previous studies47,48, strongly suggest that BacA imports these hydrophilic drugs (Extended Data Fig. 7c). Since a ΔbacA strain is not entirely resistant to aminoglycosides and tuberactinomycins, other import mechanisms must exist.
ettA mutations confer low-level resistance to diverse drugs
Another strong streptomycin-resistance hit in our screen was rv2477c, which also showed low-level resistance to other drugs (Fig. 3b,c). rv2477c is an orthologue of the Escherichia coli gene ettA (~58% amino acid identity), a ribosome-associated ABC-F protein that regulates the translation elongation cycle49,50,51. Due to its sequence similarity, we will refer to rv2477c as ettA. Biochemical studies demonstrated that ATP-bound EttA from E. coli stimulates formation of the first peptide bond of the initiating ribosome and then, concomitant with ATP hydrolysis, dissociates from the ribosome to allow translation elongation49,50. Unlike ettA in E. coli, ettA is essential in Mtb15.
Using our clinical strain genome database, we selected four non-synonymous ettA SNPs for experimental validation (Fig. 5a and Source Data Fig. 5). We also included an ettA-Trp135Gly mutation that was identified in serial Mtb isolates from a patient in Thailand directly preceding the transition from MDR-TB to extensively drug-resistant (XDR) TB52. The ettA-Trp135Gly isolate became phenotypically resistant to kanamycin and amikacin, but harboured no known resistance mutations to either aminoglycoside. All candidate SNPs were capable of complementing knockdown of the endogenous ettA allele (Fig. 5b). Both the Gly41Glu and Trp135Gly variants displayed a modest growth defect, suggesting that these two SNPs are partial loss-of-function mutations (Extended Data Fig. 7d,e). Consistent with a role for these ettA SNPs in conferring acquired drug resistance, four out of the five variants showed an increased MIC for streptomycin (Fig. 5c). The Gly41Glu and Trp135Gly strains showed >5-fold shifts in streptomycin IC50, similar in magnitude to clinically relevant gid mutants38, as well as low-level resistance to a mechanistically diverse panel of antibiotics including amikacin, ethambutol (EMB), rifampicin and levofloxacin (LVX) (Fig. 5c and Extended Data Fig. 7f,g).
To determine the mechanism by which ettA SNPs may confer low-level acquired multidrug resistance, we analysed the M. smegmatis proteome after silencing the ettA homologue, ms470015. Two of the most upregulated proteins upon ms4700 knockdown were HflX and Eis (Extended Data Fig. 7h), known members of the whiB7 regulon in Mtb35. Thus, we hypothesized that partial loss-of-function ettA alleles may promote drug resistance by stalling translation and constitutively upregulating the whiB7 stress response, in essence mimicking the effects of translation stress caused by ribosome inhibitors to activate whiB753. Consistent with this hypothesis, whiB7 and regulon genes35 were constitutively upregulated in the ettA-Gly41Glu Mtb mutant (Fig. 5d). Furthermore, simultaneous knockdown of ettA and whiB7 was able to specifically reverse aminoglycoside resistance (Fig. 5e and Extended Data Fig. 7i). whiB7 knockdown did not reverse ethambutol or levofloxacin resistance, suggesting that the mechanism by which ettA mutations confer resistance to these drugs is whiB7-independent and may instead be due to changes in translation and/or growth rates54,55.
Further epidemiological analysis focused on ettA-Gly41Glu, the most common ettA SNP in our database (n = 291, ~0.7% of all Mtb strains). Phylogenetic analysis shows that this cluster of related strains is heavily enriched for additional acquired drug resistance mutations (Fig. 5f and Source Data Fig. 5). ettA-Gly41Glu strains are found in multiple countries but are concentrated in Peru56 and indigenous communities of Colombia57, where they are associated with an MDR-TB outbreak (Fig. 5f).
A whiB7 mutation renders an Mtb sublineage sensitive to CLR
Since ettA mutations appear to confer resistance by constitutive whiB7 activation, we next mined our clinical strain genome database to identify putative gain-of-function whiB7 mutations that may be associated with acquired drug resistance58. We identified numerous putative gain-of-function mutations in the whiB7 promoter, 5’UTR, and upstream open reading frame (uORF), most of which have not been previously recognized as potential acquired drug resistance determinants (Fig. 6a and Source Data Fig. 6)58,59,60. Unexpectedly, the most common whiB7 variant in our database was a putative loss-of-function allele. This allele, whiB7 Gly64delG, represents nearly one-third (n = 851/3,186) of all whiB7 variants in our database (Fig. 6a)61,62,63. Gly64delG results in a premature stop codon and truncation of the critical DNA binding AT-hook element (Extended Data Fig. 8a)64, thus presumably inactivating WhiB7. whiB7-mediated intrinsic drug resistance typically renders macrolides ineffective in treating TB. We next sought to test whether this common Gly64delG mutation could render this subset of Mtb strains hypersusceptible to and treatable with macrolides.
Lineage calling identified the Gly64delG indel as uniquely present in all lineage 1.2.1 (L1.2.1) Mtb isolates, a major sublineage of the L1 Indo-Oceanic clade (Fig. 6a, Extended Data Fig. 8b and Source Data Fig. 6)65. Using a reference set of Mtb clinical strains66, we first confirmed the presence of the whiB7 Gly64delG indel in L1.2.1 (Fig. 6b). Consistent with loss of whiB7 function, the L1.2.1 isolate was hypersusceptible to clarithromycin as well as other macrolides, ketolides and lincosamides, whereas all other clinical isolates were intrinsically resistant (Fig. 6c and Extended Data Fig. 8c–e). The whiB7 Gly64delG allele failed to complement intrinsic clarithromycin resistance in an H37Rv ΔwhiB7 strain, confirming that Gly64delG is a loss-of-function allele (Extended Data Fig. 8f). We next tested the efficacy of clarithromycin against L1.2.1 in a low-dose aerosol mouse infection model, with drug dosing designed to mimic human pharmacokinetics67 (Extended Data Fig. 9a–d). Consistent with the in vitro results, L1.2.1 but not control strains was susceptible to clarithromycin treatment in mice (Fig.6d,e and Extended Data Fig. 9e–k)68,69.
To estimate the potential clinical impact of this finding, we next examined the geographic distribution of L1.2.1. This sublineage is found predominantly in Southeast Asia65 and is highly prevalent in the Philippines, accounting for approximately 80% of all Mtb isolates in this country70. The Philippines has one of the highest TB incidence rates in the world, including a high burden of drug-resistant TB, and TB is a leading cause of death in this country71. L1.2.1 is estimated to cause ~600,000 cases of active TB per year globally65, of which ~43,000 are estimated to be MDR-TB on the basis of the frequencies of drug resistance in our database. Thus, clarithromycin, an effective, orally available, safe and generic antibiotic, could potentially be repurposed to treat this major Mtb sublineage.
A deeper understanding of the bacterial pathways that influence drug efficacy is needed to guide TB drug development and treatment. To address this challenge, we developed a CRISPRi platform to define the determinants that influence bacterial fitness in the presence of antibiotics, and then overlayed these chemical-genetic results with comparative genomics of Mtb clinical isolates. This work builds on previous chemical-genetic efforts in Mtb3,72. Caveats include that genetic and pharmacologic target inhibition are not the same73, highlighting the importance of validating chemical-genetic interactions with small-molecule inhibitors. Moreover, all pooled screens may miss effects where the phenotype can be complemented in trans (for example cross-feeding)74. Despite these limitations, we illustrate the power of this dataset to derive clinically relevant biological insight. We uncover diverse mechanisms of intrinsic drug resistance that can be targeted to potentiate therapy, describe previously unknown mechanisms of acquired drug resistance, and make the unexpected discovery of an ‘acquired drug sensitivity’ that could enable the repurposing of clarithromycin to treat an Mtb sublineage.
We identified hundreds of genes that contribute to intrinsic drug resistance in Mtb that could serve as a foundation for the rational development of drug combinations to disarm intrinsic drug resistance. Our results confirm that one of the richest sources of potentially synergistic targets is the mycobacterial envelope3,6,7. Beyond the Mtb cell envelope, our results uncover both shared and unique intrinsic resistance and sensitivity mechanisms, as highlighted by profiling three ribosome-targeting antibiotics. Our results suggest that Rv1473 serves as an antibiotic resistance ABC-F protein, capable of displacing oxazolidinones and phenicols from the Mtb ribosome (Extended Data Fig. 6). Next-generation oxazolidinone analogues that are recalcitrant to such drug-displacing activity could be designed, analogous to third-generation tetracycline analogues which are resistant to the drug-displacing activity of the ABC-F protein TetM75. In light of our findings, we suggest designating rv1473 as ocrA (oxazolidinone chloramphenicol resistance A). Finally, these results show that trans-translation may be a target for synergistic drug combinations42, which could be important in increasing the potency and decreasing toxicity of oxazolidinones.
Discovery of previously unrecognized acquired drug resistance mechanisms will improve TB therapy by informing more effective molecular diagnostics and personalized treatment regimens. Our results illustrate the utility of combining chemical genetics with comparative genomics to power this discovery. First, we show that inhibition of tsnR increases Mtb fitness in the presence of linezolid, and thus mutations in this gene could be monitored as linezolid use is expanded in the clinic. Second, we find that loss-of-function mutations in the ABC importer bacA confer acquired drug resistance to four second-line TB drugs. Third, we show that partial loss-of-function mutations in ettA result in constitutive activation of the whiB7 stress response and low-level acquired multidrug resistance. Low-level drug resistance has been associated with TB treatment failure4, and could serve as a stepping stone to allow additional, high-level drug resistance mutations to evolve76. Our results provide a mechanistic explanation for previous findings52, whereby serial Mtb isolates from a TB patient acquired a Trp135Gly mutation in ettA directly preceding the transition from MDR to XDR-TB. Of all Mtb strains in our genome database, 3.1% harbour a missense SNP in ettA, suggesting that ettA-mediated acquired drug resistance could be common. Capreomycin remains effective against ettA variants and should be considered for treatment. Lastly, we identified numerous additional genes as candidates for mechanisms of acquired drug resistance in Mtb (Source Data Extended Fig. 7), although further work is necessary to validate these predictions.
In the search for gain-of-function whiB7 mutations that confer acquired drug resistance, we discovered common loss-of-function whiB7 alleles, a phenomenon which we refer to as ‘acquired drug sensitivity.’ Beyond whiB7, we identified several additional candidate acquired drug sensitivity alleles (Supplementary Table 2) and validate loss-of-function mmpL5 alleles in L1 and L7 isolates that render them hypersusceptible to bedaquiline and the leprosy drug clofazimine (Extended Data Fig. 10)11. Phylogenetic dating suggests that the whiB7 mutation arose approximately 900 years ago, well before the introduction of TB chemotherapy77. Since macrolides have not historically been used to treat TB, there has probably been little selective pressure against whiB7 loss-of-function mutants. It remains unclear whether the Gly64delG mutation provides or provided a selective benefit to L1.2.1, enriched as a passenger mutation, or arose as a result of genetic drift. Regardless, we find that the entire L1.2.1 sublineage is a whiB7 loss-of-function mutant which renders it susceptible to macrolides. These results pave the way for further preclinical efficacy studies to support that clarithromycin can be repurposed to treat this major Mtb sublineage.
Mtb strains are derivatives of H37Rv unless otherwise noted. A reference set of Mtb clinical strains was obtained from the Belgian Coordinated Collections of Microorganisms (BCCM)66. E. coli strains are derivatives of DH5alpha (NEB).
Mtb was grown at 37 °C in Difco Middlebrook 7H9 broth or on 7H10 agar supplemented with 0.2% glycerol (7H9) or 0.5% glycerol (7H10), 0.05% Tween-80, 1X oleic acid-albumin-dextrose-catalase (OADC) and the appropriate antibiotics (kanamycin 10–20 μg ml−1 and/or zeocin 20 μg ml−1). Anhydrotetracycline (ATc) was used at 100 ng ml−1. Mtb cultures were grown standing in tissue culture flasks (unless otherwise indicated) with 5% CO2.
Generation of individual CRISPRi and CRISPRi-resistant complementation strains
Individual CRISPRi plasmids were cloned as described in ref. 78 using Addgene plasmid 166886. Briefly, the CRISPRi plasmid backbone was digested with BsmBI-v2 (NEB R0739L) and gel purified. sgRNAs were designed to target the non-template strand of the target gene ORF. For each individual sgRNA, two complementary oligonucleotides with appropriate sticky end overhangs were annealed and ligated (T4 ligase NEB M0202M) into the BsmBI-digested plasmid backbone. Successful cloning was confirmed by Sanger sequencing.
Individual CRISPRi plasmids were then electroporated into Mtb. Electrocompetent cells were obtained as described in ref. 79. Briefly, an Mtb culture was expanded to an OD600 = 0.8–1.0 and pelleted (4,000 × g for 10 min). The cell pellet was washed three times in sterile 10% glycerol. The washed bacilli were then resuspended in 10% glycerol in a final volume of 5% of the original culture volume. For each transformation, 100 ng plasmid DNA and 100 μl electrocompetent mycobacteria were mixed and transferred to a 2 mm electroporation cuvette (Bio-Rad 1652082). Where necessary, 100 ng plasmid plRL19 (Addgene plasmid 163634) was also added. Electroporation was performed using the Gene Pulser X cell electroporation system (Bio-Rad 1652660) set at 2,500 V, 700 Ω and 25 μF. Bacteria were recovered in 7H9 for 24 h. After the recovery incubation, cells were plated on 7H10 agar supplemented with the appropriate antibiotic to select for transformants.
To complement CRISPRi-mediated gene knockdown, synonymous mutations were introduced into the complementing allele at both the protospacer adjacent motif (PAM) and the seed sequence (the 8–10 PAM-proximal bases at the 3’ end of the sgRNA targeting sequence) to prevent sgRNA targeting. Silent mutations were introduced into Gibson assembly oligos to generate ‘CRISPRi-resistant’ alleles. Complementation alleles were expressed from the endogenous or hsp60 promoters in a Tweety or Giles integrating plasmid backbone, as indicated in each figure legend and/or the plasmid descriptions. These alleles were then transformed into the corresponding CRISPRi knockdown strain, with the plRL40 Giles Int expressing plasmid where necessary. The full list of sgRNA targeting sequences and complementation plasmids can be found in Supplementary Table 2.
Pooled CRISPRi chemical-genetic screening
Chemical-genetic screens were initiated by thawing 5 ×1 ml (1 OD600 unit per ml) aliquots of the Mtb CRISPRi library15 (RLC12; Addgene 163954) and inoculating each aliquot into 19 ml 7H9 supplemented with kanamycin (10 μg ml−1) in a vented tissue culture flask (T-75; Falcon 353136). The starting OD600 of each culture was approximately 0.05. Cultures were expanded to OD600 = 1.5, pooled and passed through a 10 μm cell strainer (pluriSelect 43-50010-03) to obtain a single-cell suspension. The single-cell suspension was then treated with ATc (100 ng ml−1 final concentration) to initiate target pre-depletion. To generate 1 d pre-depletion culture, the single-cell suspension was diluted back to OD600 = 0.5 in a total volume of 40 ml 7H9. The remaining single-cell suspension was used to generate a 5 d pre-depletion culture, with a starting OD600 = 0.1 (40 ml; 100 ng ml−1 ATc). After 4 d, the 5 d pre-depletion start culture was further diluted back to a starting OD600 = 0.05 (40 ml; in 100 ng ml−1 ATc) and incubated for a further 5 d to generate the 10 d pre-depletion culture.
To initiate the chemical-genetic screen, we first collected 10 OD600 units of bacteria (~3 × 109 bacteria; ~30,000× coverage of the CRISPRi library) from the 1, 5 or 10 d CRISPRi library pre-depletion cultures as input controls. Triplicate cultures were then inoculated at OD600 = 0.05 in 10 ml 7H9 supplemented with ATc (100 ng ml−1), kanamycin (10 μg ml−1), and the indicated drug concentration or dimethyl sulfoxide (DMSO) vehicle control (Extended Data Fig. 1). Pooled CRISPRi chemical-genetic screens were performed in vented tissue culture flasks (T-25; Falcon 353109). Cultures were outgrown for 14 d at 37 °C, 5% CO2. ATc was replenished at 100 ng ml−1 at day 7. After 14 d outgrowth, OD600 values were measured for all cultures to empirically determine the MIC for each drug. Samples from three descending doses of partially inhibitory drug concentrations were processed for genomic DNA extraction, defined as ‘High’, ‘Medium’ and ‘Low’ in Extended Data Fig. 1, as described below. Due to an error during genomic DNA extraction, ethambutol 1,804 nM (‘Med’) day 1 data reflects two biological replicates, one of which was sequenced twice to produce 3 replicates. Additionally, the 10 d sample was lost for the 221 nM (‘Med’) streptomycin screen.
Genomic DNA extraction and library preparation for Illumina sequencing
Genomic DNA was isolated from bacterial pellets using the CTAB‐lysozyme method as previously described15. Briefly, Mtb pellets (5–30 OD600 units) were resuspended in 1 ml PBS + 0.05% Tween-80. Cell suspensions were centrifuged for 5 min at 4,000 × g and the supernatant was removed. Pellets were resuspended in 800 µl TE buffer (10 mM Tris pH 8.0, 1 mM EDTA) + 15 mg ml−1 lysozyme (Alfa Aesar J60701-06) and incubated at 37 °C for 16 h. Next, 70 µl 10% SDS (Promega V6551) and 5 µl proteinase K (20 mg ml−1, Thermo Fisher 25530049) were added and samples were incubated at 65 °C for 30 min. Subsequently, 100 µl 5 M NaCl and 80 µl 10% CTAB (Sigma Aldrich H5882) were added, and samples were incubated for an additional 30 min at 65 °C. Finally, 750 µl ice-cold chloroform was added and samples were mixed. After centrifugation at 16,100 × g and extraction of the aqueous phase, samples were removed from the biosafety level 3 facility. Samples were then treated with 25 µg RNase A (Bio Basic RB0474) for 30 min at 37 °C, followed by extraction with phenol:chloroform:isoamyl alcohol (pH 8.0, 25:24:1, Thermo Fisher BP1752I-400), then chloroform. Genomic DNA was precipitated from the final aqueous layer (600 µl) with the addition of 10 µl 3 M sodium acetate and 360 µl isopropanol. DNA pellets were spun at 21,300 × g for 30 min at 4 °C and washed 2× with 750 µl 80% ethanol. Pellets were dried and resuspended with elution buffer (Qiagen 19086) before spectrophotometric quantification.
The concentration of isolated genomic DNA was quantified using the DeNovix double-stranded DNA high sensitivity assay (KIT-DSDNA-HIGH-2; DS-11 series spectrophotometer/fluorometer). Next, the sgRNA-encoding region was amplified from 500 ng genomic DNA with 17 cycles of PCR using NEBNext Ultra II Q5 master mix (NEB M0544L) as described in ref. 15. Each PCR reaction contained a pool of forward primers (0.5 μM final concentration) and a unique indexed reverse primer (0.5 μM)15. Forward primers contain a P5 flow cell attachment sequence, a standard Read1 Illumina sequencing primer binding site and custom stagger sequences to guarantee base diversity during Illumina sequencing. Reverse primers contain a P7 flow cell attachment sequence, a standard Read2 Illumina sequencing primer binding site and unique barcodes to allow for sample pooling during deep sequencing.
Following PCR amplification, each ~230 bp amplicon was purified using AMPure XP beads (Beckman–Coulter A63882) using one-sided selection (1.2×). Bead-purified amplicons were further purified on a Pippin HT 2% agarose gel cassette (target range 180–250 bp; Sage Science HTC2010) to remove carry-over primer and genomic DNA. Eluted amplicons were quantified with a Qubit 2.0 fluorometer (Invitrogen), and amplicon size and purity were quality controlled by visualization on an Agilent 2100 bioanalyzer (high sensitivity chip; Agilent Technologies 5067–4626). Next, individual PCR amplicons were multiplexed into 10 nM pools and sequenced on an Illumina sequencer according to the manufacturer’s instructions. To increase sequencing diversity, a PhiX spike-in of 2.5–5% was added to the pools (PhiX sequencing control v3; Illumina FC-110-3001). Samples were run on the Illumina NextSeq 500, HiSeq 2500 or NovaSeq 6000 platform (single-read 1 ×85 cycles and 6 × i7 index cycles).
Antibacterial activity measurements
All compounds were dissolved in DMSO (VWR V0231) and dispensed using an HP D300e digital dispenser in a 384-well plate format. DMSO did not exceed 1% of the final culture volume and was maintained at the same concentration across all samples. CRISPRi strains were growth-synchronized and pre-depleted in the presence of ATc (100 ng ml−1) for 5 d before assay for MIC analysis. Cultures were then back-diluted to a starting OD580 of 0.05 and 50 µl cell suspension was plated in technical triplicate in wells containing the test compound and fresh ATc (100 ng ml−1). For checkerboard assays and MIC assays (non-CRISPRi), cultures were growth-synchronized to late log-phase and back-diluted to an OD600 of 0.025 before plating (no ATc). Plates were incubated standing at 37 °C with 5% CO2. OD600 was evaluated using a Tecan Spark plate reader at 10–14 d post-plating and percent growth was calculated relative to the DMSO vehicle control for each strain. IC50 measurements were calculated using a nonlinear fit in GraphPad Prism. For all MIC curves, data represent the mean ± s.e.m. for technical triplicates. Data are representative of at least two independent experiments.
To quantify growth phenotypes on 7H10 agar, 10-fold serial dilutions of Mtb cultures (OD600 = 0.6) were spotted on 7H10 agar containing drugs at the indicated concentrations and/or ATc at 100 ng ml−1. Plates were incubated at 37 °C and imaged after 2 weeks.
Bone marrow-derived macrophage infections
Bone marrow-derived macrophages (BMDMs) were differentiated from four wild-type, female C57BL/6NTAC mice (Taconic Farms, 6–8 weeks old). All animal work was performed in accordance with the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health, with approval from the Institutional Animal Care and Use Committee of Rockefeller University. Femurs and tibias were collected, and crushed with a sterile mortar and pestle as described80. After red blood cell lysis and counter-selection of resident macrophages, bone marrow cells were incubated in the presence of DMEM (4.5 g l−1 glucose + l-glutamine + sodium pyruvate; Corning 10–013-CV) + 10% FBS (Sigma Aldrich F4135, Lot no. 17B189) + 15% conditioned L929 cell medium (LCM) and differentiated for 7 d at 37 °C, 5% CO2. Macrophages were then lifted using gentle cell scraping. For infection assays, BMDMs were seeded in 96-well plates at 75,000 cells per well 2 d before infection. At 16 h before infection, fresh DMEM + 10% FBS + 10% LCM was added to cells, with or without IFN-γ (20 ng ml−1; Gemini Biosciences 300-311P). Mtb cultures were synchronized to late log-phase (OD600 0.6–0.8). For infections with CRISPRi strains, cultures were pre-depleted with 100 ng ml−1 ATc for 24 h before infection. Mtb pellets were washed with PBS (Thermo Fisher 14190144) + 0.05% Tyloxapol (Sigma Aldrich T0307) and single-cell suspensions were generated by collecting the suspended cells after gentle centrifugation (150 × g for 12 min). Cell culture medium was removed from the macrophages and replaced with Mtb-containing medium at a multiplicity of infection of 1:1. After 4 h of infection at 37 °C, the medium was removed and cells were washed 2× with PBS. Wells were replenished with fresh media with or without drug. DMSO was normalized to 0.2%. For CRISPRi infections, doxycycline (Sigma Aldrich D9891) was added at a concentration of 250 ng ml−1 to maintain target knockdown. For all infection assays, medium was replaced with fresh drug at day 3. At each indicated timepoint, after two PBS washes, cells were lysed with 100 µl Triton X-100 in water (Sigma Aldrich X100). Lysates were titrated in PBS + 0.05% Tween-80 and plated on 7H10 containing activated charcoal (4 g l−1) to absorb any residual ATc or antibiotic. Colony-forming units were enumerated after 21–28 d of outgrowth. Data for BMDM experiments represent the mean ± s.e.m. for technical triplicates. Results are representative of at least two independent experiments.
Selection of drug-resistant Mtb isolates
For the selection of linezolid-resistant H37Rv Mtb mutants, two independent cultures were started at an OD600 of 0.001. After 1 week of outgrowth, cultures were pelleted and roughly 3 × 109 c.f.u. were plated on 7H10 + 11.9 µM linezolid. Plates were incubated for 24 d. Colonies were picked and grown in 7H9 + 11.9 µM linezolid. Genomic DNA was collected as described above. Sanger sequencing was performed on purified PCR amplicons of rrl (23S rRNA) and rplC using the primers listed in Supplementary Table 2. Genomic DNA was also submitted for whole genome sequencing to confirm the absence of other mutations that may contribute to linezolid resistance (BGI, llumina HiSeq X Ten platform).
For selection of resistant isolates for the lineage 1.2.1 strain, 30 independent 20 ml cultures were started at an OD600 of 0.001. After growth to log-phase (OD600 0.5–0.6), cultures were pelleted and plated on 7H10 + antibiotic (CLR = 10 µg ml−1, RIF = 0.5 µg ml−1). After 28–35 d, colonies were enumerated. CLR-resistant colonies occurred at a frequency of 1.7 × 10−8 and were picked and grown in 7H9 + CLR (4 µg ml−1). Samples were heat-lysed, and whiB7 and rrl were PCR-amplified and sequenced using the primers listed in Supplementary Table 2. Sanger sequencing revealed a parental whiB7 locus (Gly64delG) in all (n = 101) clarithromycin-resistant isolates. Instead, clarithromycin resistance was conferred by a variety of base substitutions in the 23S rRNA (Extended Data Fig. 9h). Select samples were cultured further and purified genomic DNA was submitted for whole genome sequencing.
Total RNA extraction and RT-qPCR
Total RNA extraction was performed as previously described15. Briefly, 2 OD600 units of bacteria were added to an equivalent volume of GTC buffer (5 M guanidinium thiocyanate, 0.5% sodium N-lauroylsarcosine, 25 mM trisodium citrate dihydrate and 0.1 M 2-mercaptoethanol), pelleted by centrifugation, resuspended in 1 ml TRIzol (Thermo Fisher 15596026) and lysed by zirconium bead beating (MP Biomedicals 116911050). Chloroform (0.2 ml) was added to each sample and samples were frozen at −80 °C. After thawing, samples were centrifuged to separate phases and the aqueous phase was purified by Direct-zol RNA miniprep (Zymo Research R2052). Residual genomic DNA was removed by TURBO DNase treatment (Invitrogen Ambion AM2238). After RNA cleanup and concentration (Zymo Research R1017), 3 µg RNA per sample was reverse transcribed into complementary DNA (cDNA) with random hexamers (Thermo Fisher 18-091-050) following the manufacturer’s instructions. RNA was removed by alkaline hydrolysis and cDNA was purified with PCR cleanup columns (Qiagen 28115). Next, knockdown of the targets was quantified by SYBR green dye-based quantitative real-time PCR (Applied Biosystems 4309155) on a Quantstudio System 5 (Thermo Fisher A28140) using gene-specific qPCR primers (5 µM), normalized to sigA (rv2703) and quantified by the ΔΔCt algorithm. All gene-specific qPCR primers were designed using the PrimerQuest tool from IDT (https://www.idtdna.com/PrimerQuest/Home/Index) and then validated for efficiency and linear range of amplification using standard qPCR approaches. Specificity was confirmed for each validated qPCR primer pair through melting curve analysis.
Mouse infection and drug treatment
Female BALB/c mice (Charles Rivers Laboratory, 7–8 weeks old) were infected with 100–200 c.f.u. of Mtb using a whole-body inhalation exposure system (Glas-Col). After 10 d (Fig. 6d,e) or 14 d (Extended Data Fig. 9e,f), animals were randomly assigned to study groups and chemotherapy was initiated. Depending on the experiment, either 5 or 6 mice were allocated to each treatment condition (as indicated in the figure legend). Clarithromycin and rifampicin were stirred in 0.5% carboxymethylcellulose (CMC)/0.5% Tween-80 for resuspension. Isoniazid and azithromycin were resuspended in water. Liquid drug formulations were administered once daily by oral gavage for 14 consecutive days. After 13 d of drug treatment, blood samples of the mice were taken 1 h and 24 h post dosing (Extended Data Fig. 9c,d). At designated timepoints after starting chemotherapy mice were euthanized, lungs and spleens were aseptically removed, homogenized in 1 ml PBS + 0.05% Tween-80 and plated on Middlebrook 7H11 agar supplemented with 10% OADC. Colonies were counted after 4–6 weeks of incubation at 37 °C. Mice were housed in groups of 5 in individually ventilated cages inside a certified ABSL-3 facility and had access to water and food ad libitum for the duration of the study. All experiments involving animals were approved by the Institutional Animal Care and Use Committee of the Center for Discovery and Innovation.
Drug quantitation in plasma by high-pressure liquid chromatography coupled to tandem mass spectrometry (LC–MS/MS)
Neat 1 mg ml−1 DMSO stocks for rifampicin, azithromycin (AZM) and clarithromycin were serial-diluted in 50/50 (acetonitrile/water) to create neat spiking stocks. Standards and quality controls were created by adding 10 µl of spiking stock to 90 µl of drug-free plasma. Control, standard, quality control or study sample (10 µl) were added to 100 µl 50/50 (acetonitrile/methanol) protein precipitation solvent containing the stable labelled internal standards RIF-d8 (Toronto Research Chemicals R508003), AZM-d5 (Toronto Research Chemicals A927004) and CLR-13C-d3 (Cayman Chemical 26678) at 10 ng ml−1. Extracts were vortexed for 5 min and centrifuged at 1,500 × g for 5 min. The supernatant of RIF (100 µl) containing samples was combined with 5 µl 75 mg ml−1 ascorbic acid to stabilize RIF. The mixture (100 µl) was combined with 100 µl Milli-Q water before HPLC–MS/MS analysis. CD-1 mouse control plasma (K2EDTA) was sourced from Bioreclamation. RIF, AZM and CLR were sourced from Sigma Aldrich.
LC–MS/MS analysis was performed on a Sciex Applied Biosystems Qtrap 6500+ triple-quadrupole mass spectrometer coupled to a Shimadzu Nexera X2 UHPLC system to quantify each drug in plasma. Chromatography was performed on an Agilent SB-C8 (2.1 ×30 mm; particle size, 3.5 µm) using a reverse phase gradient. Milli-Q deionized water with 0.1% formic acid was used for the aqueous mobile phase and 0.1% formic acid in acetonitrile for the organic mobile phase. Multiple-reaction monitoring of precursor/product transitions in electrospray positive-ionization mode was used to quantify the analytes. Sample analysis was accepted if the concentrations of the quality control samples were within 20% of the nominal concentration. The compounds were ionized using electrospray positive-ionization mode and monitored using masses for RIF (823.50/791.60), AZM (749.38/591.30), CLR (748.38/158.20), RIF-d8 (831.50/799.60), AZM-d5 (754.37/596.30) and CLR-d4 (752.33/162.10). Data processing was performed using Analyst software (version 1.6.2; Applied Biosystems Sciex).
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The custom code used in this study is available at https://github.com/rock-lab/CGI_nature_micro_2022.
Dartois, V. The path of anti-tuberculosis drugs: from blood to lesions to mycobacterial cells. Nat. Rev. Microbiol. 12, 159–167 (2014).
Balaban, N. Q. et al. Definitions and guidelines for research on antibiotic persistence. Nat. Rev. Microbiol. 17, 441–448 (2019).
Xu, W. et al. Chemical genetic interaction profiling reveals determinants of intrinsic antibiotic resistance in Mycobacterium tuberculosis. Antimicrob. Chemother. 61, e01334-17 (2017).
Colangeli, R. et al. Bacterial factors that predict relapse after tuberculosis therapy. N. Engl. J. Med. 379, 823–833 (2018).
da Silva, P. E. A., von Groll, A., Martin, A. & Palomino, J. C. Efflux as a mechanism for drug resistance in Mycobacterium tuberculosis. FEMS Immunol. Med. Microbiol. 63, 1–9 (2011).
Batt, S. M., Minnikin, D. E. & Besra, G. S. The thick waxy coat of mycobacteria, a protective layer against antibiotics and the host’s immune system. Biochem. J. 447, 1983–2006 (2020).
Jarlier, V. & Nikaido, H. Mycobacterial cell wall: structure and role in natural resistance to antibiotics. FEMS Microbiol. Lett. 123, 11–18 (1994).
Walker, T. M. et al. Whole-genome sequencing for prediction of Mycobacterium tuberculosis drug susceptibility and resistance: a retrospective cohort study. Lancet Infect. Dis. 15, 1193–1202 (2015).
Zhang, Y., Heym, B., Allen, B., Young, D. & Cole, S. The catalase - peroxidase gene and isoniazid resistance of Mycobacterium tuberculosis. Nature 358, 591–593 (1992).
Banerjee, A. et al. inhA, a gene encoding a target for isoniazid and ethionamide in Mycobacterium tuberculosis. Science 263, 227–230 (1994).
Carter, J. J. Quantitative measurement of antibiotic resistance in Mycobacterium tuberculosis reveals genetic determinants of resistance and susceptibility in a target gene approach. Preprint at bioRxiv https://doi.org/10.1101/2021.09.14.460353 (2021).
Hicks, N. D. et al. Mutations in dnaA and a cryptic interaction site increase drug resistance in Mycobacterium tuberculosis. PLoS Pathog. 16, e1009063 (2020).
Qi, L. S. et al. Repurposing CRISPR as an RNA-guided platform for sequence-specific control of gene expression. Cell 152, 1173–1183 (2013).
Rock, J. M. et al. Programmable transcriptional repression in mycobacteria using an orthogonal CRISPR interference platform. Nat. Microbiol. 2, 16274 (2017).
Bosch, B. et al. Genome-wide gene expression tuning reveals diverse vulnerabilities of M. tuberculosis. Cell 184, 4579–4592 (2021).
Choudhary, E., Thakur, P., Pareek, M. & Agarwal, N. Gene silencing by CRISPR interference in mycobacteria. Nat. Commun. 6, 6267 (2015).
Singh, A. K. et al. Investigating essential gene function in Mycobacterium tuberculosis using an efficient CRISPR interference system. Nucleic Acids Res. 44, e143 (2016).
Li, W. et al. MAGeCK enables robust identification of essential genes from genome-scale CRISPR/Cas9 knockout screens. Genome Biol. 15, 554 (2014).
Cokol, M., Kuru, N., Bicak, E., Larkins-Ford, J. & Aldridge, B. B. Efficient measurement and factorization of high-order drug interactions in Mycobacterium tuberculosis. Sci. Adv. 3, e1701881 (2017).
Jankute, M., Cox, J. A. G., Harrison, J. & Besra, G. S. Assembly of the mycobacterial cell wall. Annu. Rev. Microbiol. 69, 405–423 (2015).
Maitra, A. et al. Cell wall peptidoglycan in Mycobacterium tuberculosis: an Achilles’ heel for the TB-causing pathogen. FEMS Microbiol. Rev. 43, 548–575 (2019).
Davis, T. D., Gerry, C. J. & Tan, D. S. General platform for systematic quantitative evaluation of small-molecule permeability in bacteria. ACS Chem. Biol. 9, 2535–2544 (2014).
Abrahams, K. A. et al. Identification of KasA as the cellular target of an anti-tubercular scaffold. Nat. Commun. 7, 12581 (2016).
Kumar, P. et al. Synergistic lethality of a binary inhibitor of Mycobacterium tuberculosis KasA. mBio 9, e02101-17 (2018).
Larrouy-Maumus, G. et al. Cell-envelope remodeling as a determinant of phenotypic antibacterial tolerance in Mycobacterium tuberculosis. ACS Infect. Dis. 2, 352–360 (2016).
Zahrt, T. C. & Deretic, V. An essential two-component signal transduction system in Mycobacterium tuberculosis. J. Bacteriol. 182, 3832–3838 (2000).
Gorla, P. et al. MtrA response regulator controls cell division and cell wall metabolism and affects susceptibility of mycobacteria to the first line antituberculosis drugs. Front. Microbiol. 9, 2839 (2018).
Nguyen, H. T., Wolff, K. A., Cartabuke, R. H., Ogwang, S. & Nguyen, L. A lipoprotein modulates activity of the MtrAB two-component system to provide intrinsic multidrug resistance, cytokinetic control and cell wall homeostasis in Mycobacterium. Mol. Microbiol. 76, 348–364 (2010).
Dejesus, M. A. et al. Comprehensive essentiality analysis of the Mycobacterium tuberculosis genome via saturating transposon mutagenesis. mBio 8, e02133-16 (2017).
Sharma, A. K. et al. MtrA, an essential response regulator of the MtrAB two-component system, regulates the transcription of resuscitation-promoting factor B of Mycobacterium tuberculosis. Microbiology 161, 1271–1281 (2015).
Peterson, E. J. et al. MtrA regulation of essential peptidoglycan cleavage in Mycobacterium tuberculosis during infection. Preprint at bioRxiv https://doi.org/10.1101/2021.02.25.432019 (2021).
Krause, K. M., Serio, A. W., Kane, T. R. & Connolly, L. E. Aminoglycosides: an overview. Cold Spring Harb. Perspect. Med. 6, a027029 (2016).
Kannan, K. et al. The general mode of translation inhibition by macrolide antibiotics. Proc. Natl Acad. Sci. USA 111, 15958–15963 (2014).
Marks, J. et al. Context-specific inhibition of translation by ribosomal antibiotics targeting the peptidyl transferase center. Proc. Natl Acad. Sci. USA 113, 12150–12155 (2016).
Morris, R. P. et al. Ancestral antibiotic resistance in Mycobacterium tuberculosis. Proc. Natl Acad. Sci. USA 102, 12200–12205 (2005).
Wilson, D. N. Ribosome-targeting antibiotics and mechanisms of bacterial resistance. Nat. Rev. Microbiol. 12, 35–48 (2014).
Madsen, C. T. et al. Methyltransferase Erm(37) slips on rRNA to confer atypical resistance in Mycobacterium tuberculosis. J. Biol. Chem. 280, 38942–38947 (2005).
Wong, S. Y. et al. Mutations in gidB confer low-level streptomycin resistance in Mycobacterium tuberculosis. Antimicrob. Agents Chemother. 55, 2515–2522 (2011).
LaMarre, J. M., Howden, B. P. & Mankin, A. S. Inactivation of the indigenous methyltransferase RlmN in Staphylococcus aureus increases linezolid resistance. Antimicrob. Agents Chemother. 55, 2989–2991 (2011).
Wasserman, S. et al. Linezolid resistance in patients with drug-resistant TB and treatment failure in South Africa. J. Antimicrob. Chemother. 74, 2377–2384 (2019).
Blondiaux, N. et al. Reversion of antibiotic resistance in Mycobacterium tuberculosis by spiroisoxazoline SMARt-420. Science 355, 1206–1211 (2017).
Alumasa, J. N. et al. Ribosome rescue inhibitors kill actively growing and nonreplicating persister Mycobacterium tuberculosis cells. ACS Infect. Dis. 3, 634–644 (2017).
Duan, W. et al. Mycobacterium tuberculosis Rv1473 is a novel macrolides ABC efflux pump regulated by WhiB7. Future Microbiol. 14, 47–59 (2019).
Sharkey, L. K. R., Edwards, T. A. & O’Neill, A. J. ABC-F proteins mediate antibiotic resistance through ribosomal protection. mBio 7, e01975 (2016).
Antonelli, A. et al. Characterization of poxtA, a novel phenicol-oxazolidinone-tetracycline resistance gene from an MRSA of clinical origin. J. Antimicrob. Chemother. 73, 1763–1769 (2018).
Personne, Y. & Parish, T. Mycobacterium tuberculosis possesses an unusual tmRNA rescue system. Tuberculosis 94, 34–42 (2014).
Domenech, P., Kobayashi, H., Levier, K., Walker, G. C. & Barry, C. E. BacA, an ABC transporter involved in maintenance of chronic murine infections with Mycobacterium tuberculosis. J. Bacteriol. 191, 477–485 (2009).
Rempel, S. et al. A mycobacterial ABC transporter mediates the uptake of hydrophilic compounds. Nature 580, 409–412 (2020).
Boël, G. et al. The ABC-F protein EttA gates ribosome entry into the translation elongation cycle. Nat. Struct. Mol. Biol. 21, 143–151 (2014).
Chen, B. et al. EttA regulates translation by binding the ribosomal E site and restricting ribosome-tRNA dynamics. Nat. Struct. Mol. Biol. 21, 152–159 (2014).
Cui, Z. et al. Interplay between an ATP-binding cassette F protein and the ribosome from Mycobacterium tuberculosis. Nat. Commun. 13, 432 (2022).
Faksri, K. et al. Whole-genome sequencing analysis of serially isolated multi-drug and extensively drug resistant Mycobacterium tuberculosis from Thai patients. PLoS ONE 11, e0160992 (2016).
Schrader, S. M. et al. Multiform antimicrobial resistance from a metabolic mutation. Sci. Adv. 7, eabh2037 (2021).
Brito, L. et al. Absence of tmRNA has a protective effect against fluoroquinolones in Streptococcus pneumoniae. Front. Microbiol. 7, 2164 (2017).
Lobritz, M. A. et al. Antibiotic efficacy is linked to bacterial cellular respiration. Proc. Natl Acad. Sci. USA 112, 8173–8180 (2015).
Sheen, P. et al. Genetic diversity of Mycobacterium tuberculosis in Peru and exploration of phylogenetic associations with drug resistance. PLoS ONE 8, e65873 (2013).
Marín, A. V., Rastogi, N., Couvin, D., Mape, V. & Murcia, M. I. First approach to the population structure of Mycobacterium tuberculosis complex in the indigenous population in Puerto Nariño-Amazonas, Colombia. PLoS ONE 16, e0245084 (2021).
Reeves, A. Z. et al. Aminoglycoside cross-resistance in Mycobacterium tuberculosis due to mutations in the 5’ untranslated region of whiB7. Antimicrob. Agents Chemother. 57, 1857–1865 (2013).
Kaur, S. et al. Novel mutations conferring resistance to kanamycin in Mycobacterium tuberculosis clinical isolates from Northern India. Tuberculosis 96, 96–101 (2016).
Chakravorty, S. et al. Genotypic susceptibility testing of Mycobacterium tuberculosis isolates for amikacin and kanamycin resistance by use of a rapid sloppy molecular beacon-based assay identifies more cases of low-level drug resistance than phenotypic Lowenstein-Jensen testing. J. Clin. Microbiol. 53, 43–51 (2015).
Merker, M. et al. Phylogenetically informative mutations in genes implicated in antibiotic resistance in Mycobacterium tuberculosis complex. Genome Med. 12, 27 (2020).
Vargas, R. et al. Role of Epistasis in Amikacin, Kanamycin, Bedaquiline, and Clofazimine Resistance in Mycobacterium tuberculosis Complex. Antimicrob. Agents Chemother. 65, e0116421 (2021).
Warit et al. Genetic characterisation of a whiB7 mutant of a Mycobacterium tuberculosis clinical strain. J. Glob. Antimicrob. Resist. 3, 262–266 (2015).
Burian, J. et al. The mycobacterial antibiotic resistance determinant WhiB7 acts as a transcriptional activator by binding the primary sigma factor SigA (RpoV). Nucleic Acids Res. 41, 10062–10076 (2013).
Netikul, T., Palittapongarnpim, P., Thawornwattana, Y. & Plitphonganphim, S. Estimation of the global burden of Mycobacterium tuberculosis lineage 1. Infect. Genet. Evol. 91, 104802 (2021).
Borrell, S. et al. Reference set of Mycobacterium tuberculosis clinical strains: a tool for research and product development. PLoS ONE 14, e0214088 (2019).
Rodvold, K. A. Clinical pharmacokinetics of clarithromycin. Clin. Pharmacokinetics 37, 385–398 (1999).
Truffot-Pernot, C., Lounis, N., Grosset, J. H. & Ji, B. Clarithromycin is inactive against Mycobacterium tuberculosis. Antimicrob. Agents Chemother. 39, 2827–2828 (1995).
Luna-Herrera, J., Reddy, V. M., Daneluzzi, D. & Gangadharam, P. R. Antituberculosis activity of clarithromycin. Antimicrob. Agents Chemother. 39, 2692–2695 (1995).
Phelan, J. E. et al. Mycobacterium tuberculosis whole genome sequencing provides insights into the Manila strain and drug-resistance mutations in the Philippines. Sci. Rep. 9, 9305 (2019).
Global Tuberculosis Report (WHO, 2021).
Johnson, E. O. et al. Large-scale chemical genetics yields new M. tuberculosis inhibitor classes. Nature 571, 72–78 (2019).
Knight, Z. A. & Shokat, K. M. Chemical genetics: where genetics and pharmacology meet. Cell 128, 425–430 (2007).
Thibault, D. et al. Droplet Tn-Seq combines microfluidics with Tn-Seq for identifying complex single-cell phenotypes. Nat. Commun. 10, 5729 (2019).
Jenner, L. et al. Structural basis for potent inhibitory activity of the antibiotic tigecycline during protein synthesis. Proc. Natl Acad. Sci. USA 110, 3812–3816 (2013).
Dick, T. & Dartois, V. TB drug susceptibility is more than MIC. Nat. Microbiol. 3, 971–972 (2018).
O’Neill, M. B. et al. Lineage specific histories of Mycobacterium tuberculosis dispersal in Africa and Eurasia. Mol. Ecol. 28, 3241–3256 (2019).
Wong, A. I. & Rock, J. M. CRISPR interference (CRISPRi) for targeted gene silencing in mycobacteria. Methods Mol. Biol. 2314, 343–364 (2021).
Murphy, K. C., Papavinasasundaram, K. & Sassetti, C. M. Mycobacterial recombineering. Methods Mol. Biol. 1285, 177–199 (2015).
Trouplin, V. et al. Bone marrow-derived macrophage production. J. Vis. Exp. 81, e50966 (2013).
Shell, S. S. et al. Leaderless transcripts and small proteins are common features of the mycobacterial translational landscape. PLoS Genet. 11, e1005641 (2015).
We thank members of the Rock laboratory, S. Ehrt, J. Pritchard, A. Gouzy and S. Grover for comments on the manuscript and/or helpful discussions; C. Trujillo, J. Wallach, S. Lavalette-Levi and S. Ehrt for technical assistance, J. Xiang and D. Xu of the Weill Cornell Genomics Core for sequencing; the animal technical and analytical teams of the Center for Discovery and Innovation for animal work; R. Froom and V. LaSalle for scientific illustration; and S. Schrader and C. Barry for sharing bacterial strains. This work was supported by a Harvey L. Karp Postdoctoral Fellowship (S.L.), the Potts Memorial Foundation (M.A.D. and S.L.), the Bill and Melinda Gates Foundation (INV-010616 and INV-004761, D.S.), the Department of Defense (PR192421, J.M.R.), the Robertson Therapeutic Development Fund (J.M.R.), an NIH Shared Instrumentation Grant (S10-OD023524, V.A.D.) and an NIH/NIAID New Innovator Award (1DP2AI144850-01, J.M.R.).
All authors declare no competing interests.
Peer review information
Nature Microbiology thanks Clifton Barry, Luiz Pedro de Carvalho and the other, anonymous, reviewer(s) 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.
a-i, Normalized growth (mean ± SEM, n = 3 biological replicates) of the Mtb CRISPRi library in the drug screens. Samples harvested for sgRNA deep sequencing are marked as “High”, “Med”, and “Low”, denoting the three descending doses of partially inhibitory drug concentrations analyzed in these screens. **: 10-day sample was lost for the 221 nM (“Med”) streptomycin screen. One biological replicate was lost for the 1,804 nM (“Med”) EMB 1-day screen; to obtain three replicate samples, one biological replicate was prepared in technical duplicate.
a, Histogram depicting the number of unique chemical-genetic interactions for enriching and depleting hits. Hit genes were defined as the union of 1 and 5-day CRISPRi library pre-depletion results. b-j, Bar graphs showing the number of hit genes identified across all drugs. Gene essentiality calls were defined by CRISPRi15. D1, D5, and D10 indicate the number of days the CRISPRi library was treated with ATc prior to drug exposure; D1 + 5 = hit genes defined as the union of 1 and 5-day CRISPRi library pre-depletion results; D1 + 5 + 10: hit genes defined as the union of 1, 5 and 10 day CRISPRi library pre-depletion results. The 10-day sample was lost for the “Med” streptomycin screen and thus the D10 containing results for “STR–Med” are labelled “missing”. BDQ = bedaquiline; CLR = clarithromycin; EMB = ethambutol; INH = isoniazid; LVX = levofloxacin; LZD = linezolid; RIF = rifampicin, STR = streptomycin; VAN = vancomycin.
a, Heatmap of odds-ratios showing enrichment of essential gene targeting sgRNAs as hits in the chemical-genetic screen. A Fisher’s exact test was used to evaluate enrichment of essential gene targeting sgRNAs relative to non-essential gene targeting sgRNAs amongst hit genes (FDR < 0.01, |L2FC | > 1) in the chemical genetic screen. BDQ = bedaquiline; CLR = clarithromycin; EMB = ethambutol; INH = isoniazid; LVX = levofloxacin; LZD = linezolid; RIF = rifampicin, STR = streptomycin; VAN = vancomycin. b, Heatmap showing clustered chemical-genetic profiles from the 5-day CRISPRi library pre-depletion screen. Genes are clustered along the vertical axis; for simplicity, only genes that hit in at least two drug conditions are shown (n = 676 genes). Ascending drug concentrations (“Low”, “Med”, “High” indicated by white triangles) are clustered along the horizontal axis. The median L2FC for each gene following drug selection (relative to vehicle control) is indicated on the color scale. If a gene was not a significant hit (FDR > 0.01), the L2FC value was plotted as 0 for the corresponding condition. c, Bar plots of the enriched (P < 0.05) KEGG categories for hit genes for the indicated drugs. KEGG annotations were manually updated to include the mycolic acid-arabinogalactan-peptidoglycan (mAGP) complex-associated genes described in20,21. d, Correlation of mAGP signature and drug physiochemical properties. For each drug, the L2FC distribution (“High” concentration, 5-day CRISPRi library pre-depletion) is shown for a select group of 78 genes involved in mAGP assembly and regulation as described in20,21. L2FC values (mean ± SEM, n = 3 biological replicates) for the 78 genes under each drug treatment are shown. For each condition, the box indicates the lower quartile, median, and upper quartile and whiskers represent the minimum and maximum L2FC values.
a, Diagram of the mycobacterial mAGP complex. Select genes involved in mycolic acid synthesis and transport (kasAB, mmpL3), arabinogalactan biosynthesis (embAB, dprE1), and peptidoglycan remodeling (ponA2, ripA) are highlighted. b, Heatmap of chemical-genetic hit genes from the 5-day CRISPRi library pre-depletion screen. The color of each circle represents the gene-level L2FC. A white dot represents an FDR < 0.01 and a | L2FC | > 1. ilvC and ccdA are included as non-hit controls. c,d, Single strain validation of mAGP-associated hits. Dose-response curves (c, mean ± SEM, n = 3 biological replicates) for the indicated hypomorphic CRISPRi strains. Growth curves (d, mean ± SEM, n = 3 biological replicates) are derived from the vehicle control samples. NT = non-targeting; KD = knockdown. e,f, KasA inhibitor (GSK’724 A) checkerboard assays to quantify drug-drug interactions. Dose-response curves (f, mean ± SEM, n = 3 biological replicates) are shown for each drug in the absence (DMSO) or presence of 0.25X MIC80 GSK’724 A. The fractional inhibitory concentration index (FICI) values listed represent the lowest value obtained from each checkerboard assay. g, GSK’724 A synergy with rifampicin in resting and IFN-γ-activated murine bone marrow derived macrophages (mean CFU/ml ± SEM, n = 3 biological replicates). Results from an unpaired, two-tailed t-test are shown. h,i, Ethidium bromide (h) and Vancomycin-BODIPY (i) uptake (mean ± SEM, n = 4 biological replicates) of H37Rv pre-treated for two days with DMSO or subinhibitory linezolid, GSK’724 A, or ethambutol. Results from an unpaired, two-tailed t-test are shown.
a, Time-kill curves (mean ± SEM, n = 3 biological replicates) for the indicated CRISPRi strains. NT = non-targeting; KD = knockdown; CR = CRISPRi-resistant. b, Growth (mean ± SEM, n = 3 biological replicates) of the indicated CRISPRi strains in resting murine bone marrow derived macrophages. Significance was determined by two-way ANOVA and adjusted for multiple comparisons. ***, p < 0.001; ****, p < 0.0001. c, Dose-response curves (mean ± SEM, n = 3 biological replicates) for the indicated strains. d, Circos plot depicting overlapping genes identified by RNA-seq (Fig. 2f) and MtrA ChIP-seq27. Outer track: the H37Rv genome by nucleotide position; middle track: lines mark genes with significant L2FC values (padj < 0.05) upon mtrA knockdown (blue = positive L2FC; red = negative L2FC); inner tracks: black lines mark genes defined as interacting with MtrA by ChIP-seq27, and grey lines highlight genes which display both a significant expression change (padj < 0.05; |L2FC | > 1) by mtrA RNAseq and are found to interact with MtrA by ChIP-seq. e, Identification of an MtrA consensus binding motif. MEME analysis was performed on the promoter regions of candidate genes found to be downregulated upon mtrA silencing and bound by MtrA by ChIP-seq27 (n = 25 genes). f,g, Quantification (mean ± SEM, n = 3 biological replicates) of gene mRNA levels by qRT-PCR. Strains were grown + /– ATc for ~3 generations prior to harvesting RNA. Statistical significance was calculated as p-value with unpaired t-test. *, p < 0.05; **, p < 0.01; ***, p < 0.001. h, Quantification (mean ± SEM, n = 3 biological replicates) of gene mRNA levels by qRT-PCR. Wild-type H37Rv was grown in the presence of the indicated stress (RIF/BDQ/INH: 4X IC50, SDS: 0.2%, DMSO: 0.5%) for 3 hours prior to harvesting RNA. Statistical significance was calculated as p-value with unpaired T-test. ***, p < 0.001.
Extended Data Fig. 6 Mtb encodes diverse mechanisms of intrinsic resistance to ribosome-targeting antibiotics.
a, Ethambutol checkerboard assays to quantify drug-drug interactions. Dose-response curves (mean ± SEM, n = 3 biological replicates) are shown for each drug in the absence (DMSO) or presence of 0.25X MIC80 of EMB. Fractional inhibitory concentration index (FICI) values listed represent the lowest value obtained from each checkerboard assay. b, Phylogenetic tree of antibiotic resistance (ARE) ABC-F proteins from the indicated species. Figure adapted from44 Bootstrap values (500 replicates) are indicated at each node. c, Growth curves for the linezolid-associated hit genes and control strains shown in Fig. 3d. Curves (mean ± SEM, n = 3 biological replicates) are derived from the vehicle control samples of the MIC assay. NT = non-targeting; KD = knockdown. d, Dose-response curves (mean ± SEM, n = 3 biological replicates) were measured for CRISPRi knockdown strains targeting smpB and clpP2 in wild-type H37Rv. e, Growth curves for the strains shown in panel (d). Curves (mean ± SEM, n = 3 biological replicates) are derived from the vehicle control samples of the MIC assay. f, Dose-response curves (mean ± SEM, n = 6 biological replicates) of WT H37Rv and an isogenic rplC-Cys154Arg mutant. g, Dose-response curves (mean ± SEM, n = 3 biological replicates) for the indicated CRISPRi strains.
a, Dose-response curves (mean ± SEM, n = 3 biological replicates) show that the Val118Ala and Asp546Ala mutations in bacA do not confer drug resistance. KO = knockout; EV = empty complementation vector. b, Overexpression of Mtb bacA confers streptomycin sensitivity in M. smegmatis. Dose-response curves (mean ± SEM, n = 3 biological replicates) for the indicated strains. c, LogP values for the antibiotics to which bacA mutants show an increased MIC (streptomycin, amikacin, capreomycin, kanamycin) or no MIC change (rifampicin, ethambutol, levofloxacin, linezolid). Results from an unpaired t-test are shown: ***, p < 0.001. d, Growth curves for the strains shown in Fig. 5c. Curves (mean ± SEM, n = 3 biological replicates) are derived from the vehicle control samples of the MIC assay. KD = knockdown. e, Sequence alignment for EttA orthologs from the indicated species for the region surrounding the N-terminal Walker A motif. The Mtb EttA Gly41 residue is boxed. Accession numbers are listed next to each species. f, Dose-response curves (mean ± SEM, n = 3 biological replicates) for the strains shown in Fig. 5c.g, Dose-response curves (mean ± SEM, n = 3 biological replicates) show that the Pro39Ser mutation in ettA does not confer drug resistance. h, Quantitative mass spectrometry results following CRISPRi knockdown of ms4700 (described in15). Data represent protein level fold-change (mean ± SEM, n = 4 technical replicates derived from 2 biological replicates). Ms4700 could only be detected in two +ATc replicates and thus the mean ± SEM for duplicates is shown. i, Growth curves for the strains shown in Fig. 5e. Curves (mean ± SEM, n = 3 biological replicates) are derived from the vehicle control samples of the MIC assay.
Extended Data Fig. 8 L1.2.1 is a whiB7 loss-of-function mutant and hypersusceptible to macrolides, ketolides, and lincosamides.
a, Alignment of WhiB7 orthologues from representative actinobacteria. Accession numbers are listed next to each species. The conserved glycine-rich motif and DNA binding AT-hook element are highlighted. b, Phylogenetic tree of all L1 Mtb clinical isolates (n = 3,408) in our genome database (Source Data Fig. 4). L1.2.1 and the whiB7 Gly64delG mutation are highlighted. c-e, Dose-response curves (mean ± SEM, n = 3 biological replicates) for a reference set of Mtb clinical strains66. f, H37Rv or a ΔwhiB7 H37Rv strain were transformed with an integrating plasmid to express either the H37Rv whiB7 allele or the L1.2.1 whiB7 Gly64delG allele in trans from its native promoter. Dose-response curves (mean ± SEM, n = 3 biological replicates) for the resulting strains are shown.
a,b, Growth of H37Rv and L1.2.1 in vivo. BALB/c mice were infected with approximately 100-200 c.f.u. by aerosol. Mtb burden (mean c.f.u. ± SEM) in lungs (a) and spleens (b) was determined at the indicated timepoints. Data represent 3 mice at D0 (lung only), 5 mice at D14 and D28, and 6 mice at D56. c,d, Plasma drug concentrations (mean ± SD for 4 mice) after 2 weeks of drug therapy. Blood was collected at 1 h (c) and 24 h (d) post-dose after 13 daily doses from vehicle control (VC) and treatment groups further described in (e,f). Drug concentrations were measured in plasma using high pressure liquid chromatography coupled to tandem mass spectrometry. AZM = azithromycin; CLR = clarithromycin; RIF = rifampicin. e,f, Lung (e) and spleen (f) Mtb burden (mean c.f.u. ± SEM, n = 5 mice) in BALB/c mice after azithromycin (200 mg/kg), clarithromycin (200 mg/kg), or rifampicin (25 mg/kg) treatment. Mice were infected with approximately 100-200 c.f.u. of aerosolized Mtb. After two weeks to allow the acute infection to establish, chemotherapy was initiated. Following two weeks of drug therapy, Mtb bacterial load was determined. Statistical significance was assessed by one-way ANOVA followed by Tukey’s post-hoc test. *, p < 0.05; ****, p < 0.0001. g, Rifampicin and clarithromycin mutation frequency analysis with the L1.2.1 strain. Results from an unpaired, two-tailed student’s t-test are shown h, Distribution of 23 S rRNA mutations from in vitro-selected, clarithromycin-resistant L1.2.1 isolates from (g). i, Dose-response curves (mean ± SEM, n = 3 biological replicates) of representative CLR-resistant (CLRR) L1.2.1 isolates. j,k, Lung (j) and spleen (k) Mtb burden (mean c.f.u. ± SEM) in BALB/c mice after isoniazid (INH; 25 mg/kg) or clarithromycin (200 mg/kg) treatment. Mice were infected with approximately 100-200 c.f.u. of aerosolized Mtb. After ten days to allow the acute infection to establish, chemotherapy was initiated. Mtb bacterial load was determined at the indicated time points. Data represent 3 mice at D0 (lung only) and 6 mice at D10 and D24.
Extended Data Fig. 10 Some Mtb clinical strains have loss-of-function mmpL5 mutations that render them hypersensitive to bedaquiline and clofazimine.
Dose-response curves (mean ± SEM, n = 3 biological replicates) for a reference set of Mtb clinical strains66. b, Dose-response curves (mean ± SEM, n = 3 biological replicates) for the listed Mtb strains. The L1.1 strain (mmpL5 Tyr300Stop) in panel a was transformed with an integrating plasmid expressing either an empty vector (EV) or the mmpS5 + mmpL5 operon driven by the endogenous (pNative) or hsp60 promoter.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
Statistical source data.
About this article
Cite this article
Li, S., Poulton, N.C., Chang, J.S. et al. CRISPRi chemical genetics and comparative genomics identify genes mediating drug potency in Mycobacterium tuberculosis. Nat Microbiol 7, 766–779 (2022). https://doi.org/10.1038/s41564-022-01130-y
This article is cited by
The evolution of antibiotic resistance is associated with collateral drug phenotypes in Mycobacterium tuberculosis
Nature Communications (2023)
Nature Biotechnology (2023)
Structural basis for triacylglyceride extraction from mycobacterial inner membrane by MFS transporter Rv1410
Nature Communications (2023)
Scientific Reports (2023)
Nature Microbiology (2022)