DNA-Dependent Binding of Nargenicin to DnaE1 Inhibits Replication in Mycobacterium tuberculosis

Abstract

Natural products provide a rich source of potential antimicrobials for treating infectious diseases for which drug resistance has emerged. Foremost among these diseases is tuberculosis. Assessment of the antimycobacterial activity of nargenicin, a natural product that targets the replicative DNA polymerase of Staphylococcus aureus, revealed that it is a bactericidal genotoxin that induces a DNA damage response in Mycobacterium tuberculosis (Mtb) and inhibits growth by blocking the replicative DNA polymerase, DnaE1. Cryo-electron microscopy revealed that binding of nargenicin to Mtb DnaE1 requires the DNA substrate such that nargenicin is wedged between the terminal base pair and the polymerase and occupies the position of both the incoming nucleotide and templating base. Comparative analysis across three bacterial species suggests that the activity of nargenicin is partly attributable to the DNA binding affinity of the replicative polymerase. This work has laid the foundation for target-led drug discovery efforts focused on Mtb DnaE1.

Claiming an estimated 1.5 million lives in 2020, tuberculosis (TB) remains one of the leading causes of death globally from an infectious disease.¹ The severe disruptions to health services wrought by the COVID-19 pandemic are predicted to worsen this grim toll by a further 1 million TB deaths per annum over the next four years.¹ In the absence of a highly efficacious vaccine, prolonged chemotherapy with combinations of anti-TB drugs forms the cornerstone of TB control. However, the increase of drug resistance through ongoing evolution and spread of drug-resistant strains of the etiologic agent, Mycobacterium tuberculosis (Mtb), is undermining current efforts. This problem, exacerbated by additional treatment delays caused by the pandemic, underscores the urgent need for new TB drugs with distinct mechanisms of action for inclusion in shorter, safer, and more effective drug regimens. The TB drug discovery and development pipeline established in recent years has begun to deliver new and repurposed drugs and combinations that have revolutionized the treatment of drug-resistant TB² and demonstrated that treatment shortening is an achievable goal.³ However, maintaining this momentum requires replenishment of the pipeline with high-quality hit compounds that show mechanistic novelty.⁴ This is a key objective of the Tuberculosis Drug Accelerator (TBDA).⁵

Of the vital cellular processes targeted by TB drugs in clinical use, DNA replication stands out as relatively under-represented;⁶⁻⁸ this is despite the high vulnerability of some genes essential for DNA replication in Mtb,⁹ including those encoding DNA gyrase, the target of the fluoroquinolones, moxifloxacin, gatifloxacin, and levofloxacin, and the only DNA metabolic enzyme currently targeted for TB therapy. Fluoroquinolones inhibit DNA gyrase with bactericidal consequences for Mtb(10,11) and have been incorporated in second-line therapy for multidrug-resistant (MDR) TB¹² and in treatment-shortening regimens for drug-susceptible TB.³ The identification of novel scaffolds that target DNA gyrase remains an active area of investigation,^13,14 while topoisomerase I is also being pursued as a new TB drug target.¹⁵ Recently, the replisome—the macromolecular machine that copies the bacterial chromosome—has emerged as an attractive target for TB^6,7 and antibacterial drug discovery, more generally.¹⁶ Key discoveries involving natural products have added impetus to exploring this target further: first, griselimycin, a cyclic depsipeptide discovered more than 50 years ago, was shown to bind with high affinity and selectivity to the β-clamp (DnaN) at the site of interaction with DNA polymerase and other DNA metabolizing enzymes.¹⁷ During DNA replication, the β-clamp interacts with DnaE1, the replicative DNA polymerase termed variously as DnaE, DnaE1, or PolC in different bacteria, greatly enhancing the processivity of the polymerase. Griselimycin interferes with the protein interaction between DnaE1 and the β-clamp, affecting the processivity of DNA replication.¹⁷ The mechanistic novelty of griselimycin led to the development of the analogue, cyclohexyl-griselimycin, which has improved potency and stability and demonstrated comparable efficacy to rifampicin when used in combination with first-line drugs in a mouse infection model.¹⁷ Second, studies in Staphylococcus aureus identified the replicative DNA polymerase, DnaE, as the target of nargenicin A1 (referred to here as nargenicin),¹⁸ which belongs to a class of partially saturated alicyclic polyketides comprising an octalin ring (Figure 1A).¹⁹ Nargenicin is an ether-bridged macrolide antibiotic first isolated from various Nocardia species almost three decades ago.^20,21 It is a narrow-spectrum antimicrobial¹⁸ with activity against gram-positive bacteria, including methicillin-resistant S. aureus and Micrococcus luteus.²² The identification of narR/ngnU,^21,23 a dnaE homologue immediately adjacent to the nargenicin biosynthetic gene cluster in the producer organism, Nocardia sp. CS682,²⁴ suggested a mechanism of self-resistance to nargenicin using NarR/NgnU as a “decoy”.²¹

Figure 1.

Antimycobacterial activity profile of nargenicin. (A) Chemical structure of nargenicin A1. (B) Antibacterial activity (minimal inhibitory concentration, MIC) of nargenicin (NRG) in mycobacteria and other organisms illustrating the effect of media composition on activity. 7H9, Middlebrook 7H9 media; GAST/(Fe), glycerol-alanine-salts (with iron); Glu, glucose; (O)ADC, (oleic acid)-albumin-dextrose-catalase; Tw, Tween-80; Tx, Tyloxapol. (C) Time–kill kinetics of nargenicin in Mtb, measured by CFU enumeration. Error bars represent the SD derived from two biological replicates. Ciprofloxacin (CIP; MIC = 1.5 μM) was used as a comparator. (D) Drug-induced lytic activity measured by the release of GFP from Mtb H37Rv-GFP at the indicated concentrations.³² Linezolid (LIN; MIC = 1.5 μM) and meropenem (MERO; MIC = 5.2 μM) were used as the nonlytic and lytic controls, respectively. Data are representative of the two biological replicates.

The potent bactericidal activity and low frequency of resistance for nargenicin in S. aureus(18) led us to investigate the antimycobacterial properties of this molecule²⁵ under the auspices of the TBDA. Here, we show that nargenicin is a bactericidal genotoxin that induces a DNA damage response in Mtb that is accompanied by cellular elongation and potential weakening of the cell envelope. We further demonstrate that the antimycobacterial activity of nargenicin is mediated through the inhibition of DNA synthesis, consistent with the inhibition of the DNA polymerase activity of purified DnaE1. Structural analysis by cryo-electron microscopy (cryo-EM) revealed a unique mode of binding by nargenicin to Mtb DnaE1 in the presence of DNA in which nargenicin occupies the position of both the incoming nucleotide and templating base and stacks onto the terminal base pair. We show that the antibacterial efficacy of nargenicin as a DNA replication inhibitor is attributable, at least in part, to the DNA binding affinity of the organism’s replicative polymerase.

Results

Nargenicin is Bactericidal against Mtb In Vitro

Nargenicin was shown to have a minimum inhibitory concentration (MIC) of 12.5 μM against Mtb H37Rv under standard culture conditions (7H9/OADC/Tw) (Figure 1B; Table S1). In this culture medium, nargenicin showed comparable activity against a range of drug-sensitive and drug-resistant clinical isolates of Mtb and was active against Mycobacterium smegmatis (Msm). The activity against Mtb diminished significantly when Tween-80 was replaced by Tyloxapol to disperse the mycobacteria. A synergistic effect of Tween-80 has been observed for other TB drugs, most notably rifampicin²⁶ and streptomycin.²⁷ The differential potency of nargenicin in media containing Tween-80 versus Tyloxapol likely reflects the differential impact of these two detergents on the lipid composition of the cell envelope at the concentrations typically used for clump dispersal²⁸ with Tween-80 increasing permeability to the drug.^29,30 Nargenicin also showed increased potency in GAST/(Fe)/Tween-80. The in vitro selectivity index was reasonable with limited cytotoxicity against the HepG2 cell line (CC50 > 100 μM).

Time–kill kinetic analysis revealed that nargenicin was bactericidal in Mtb H37Rv, showing time-dependent kill with limited dose-dependency over the concentration range tested (Figure 1C). To ascertain whether this bactericidal activity was accompanied by cell lysis, we quantified green fluorescent protein (GFP) release from H37Rv-GFP.^31,32 Nargenicin treatment led to GFP release from day 4 onwards, peaking on days 6–7 (Figure 1D). Griselimycin treatment also resulted in delayed GFP release analogous to that elicited by nargenicin, but no release of GFP was observed upon exposure to the DNA gyrase inhibitors, ciprofloxacin, or moxifloxacin, demonstrating that the GFP release was not a generic consequence of disrupting DNA metabolism (Figure 1D).

Nargenicin Inhibits DNA Synthesis and is Genotoxic in Mtb

To ascertain whether nargenicin shares the same mechanism of action in mycobacteria as in S. aureus,¹⁸ we applied a suite of complementary biological profiling assays in Mtb and Msm. Multiple attempts to isolate spontaneous nargenicin-resistant mutants in Mtb or Msm by plating 10⁹–10¹⁰ bacilli on media containing nargenicin at 5–20× MIC (Mtb) or 1–10× MIC (Msm) were unsuccessful, yielding no heritably resistant mutants. Reasoning that nargenicin would elicit a DNA damage response if it disrupts DNA replication, we used the Mtb PrecA-LUX reporter strain to monitor the activity of the DNA-damage-inducible recA promoter in response to drug treatment.³³ Like fluoroquinolones and griselimycin, nargenicin triggered dose-dependent induction of luminescence (Figures 2A and S1). Comparative DNA microarray analysis revealed a transcriptomic signature for nargenicin-treated Mtb that shared key features with those elicited by mitomycin C and fluoroquinolones (Figures S2A, S2B, and Table S2).^34,35 Genome-wide transcriptome analysis by RNA-seq revealed a profound upregulation of dnaE2, imuA′, and imuB, components of the mycobacterial “mutasome” responsible for DNA damage tolerance and damage-induced mutagenesis^35,36 and other DNA repair and recombination genes, including recA, radA, uvrA, lhr, and adnAB (Figures 2B, S2C, and Data S1), which are contained in the PafBC regulon.³⁷ Interestingly, deletion of either recA(38) or dnaE2(35,36) had a negligible impact on the antimycobacterial activity of nargenicin (Table S1). Genes most highly downregulated by nargenicin were enriched in those associated with cell division (ftsZ, whiB2, and ripA) and included genes involved in cell envelope biogenesis (e.g., fbpC) (Figures 2B and S2C).

Figure 2.

Nargenicin is a genotoxin that inhibits DNA replication in mycobacteria. (A) Analysis of recA promoter activity elicited by nargenicin using the reporter strain, PrecA-LUX.³³ Ciprofloxacin (CIP, 2× MIC) was a positive control. RLU, relative luminescence units. (B) Volcano plot illustrating the transcriptional response (RNA-seq) of Mtb to nargenicin (10× MIC). Differential expression (Log 2 fold-change) of nargenicin-treated cultures versus dimethyl sulfoxide (DMSO)-treated controls are plotted against adjusted P-values (P-value) for each gene, indicating a significant upregulation of genes involved in the response of Mtb to DNA-damaging agents.³⁵ (C) Morphological profiling of Msm in response to treatment with nargenicin illustrates that bacillary morphotypes³⁹ cluster in UMAP space with those of CRISPRi hypomorphs in genes involved in DNA replication, including dnaE1. Black circle, untreated; black square, DMSO-treated; red circle, nargenicin-treated at 1× MIC; red square, nargenicin-treated at 2× MIC; and red triangle, nargenicin-treated 4× MIC. (D) Selective inhibition of DNA synthesis by nargenicin in Mtb. The incorporation of radiolabeled precursors into the total nucleic acid (tNA), protein (Prot), peptidoglycan (PG), and fatty acid (FA) was measured in the absence (DMSO) or presence of nargenicin at 2× or 20× MIC (black and red bars, respectively). The level of radiolabel incorporation into each macromolecular species is depicted relative to the DMSO-treated control. Assay specificity was confirmed using the following pathway-specific antibiotics as positive controls: ofloxacin (DNA replication; 5 μg/mL), streptomycin (protein synthesis; 10 μg/mL), d-cycloserine (peptidoglycan biosynthesis; 5 μg/mL), and isoniazid (fatty acid biosynthesis; 0.2 μg/mL). Error bars represent the standard deviations from two experimental repeats.

Morphological profiling of Msm exposed to nargenicin revealed a filamentation phenotype with the proportion of elongated bacilli in the population increasing with the drug dose (Figure S3). This drug-induced profile clustered closely in UMAP space with those resulting from transcriptional silencing of components of the DNA replication and repair machinery (Figure 2C), as previously defined,³⁹ further implicating the disruption of DNA metabolism in the mode of action of nargenicin. Direct evidence for the inhibition of DNA replication was then obtained from a macromolecular incorporation assay, which compares the incorporation of radiolabeled precursors into the total nucleic acid, DNA, protein, peptidoglycan, or fatty acid in cells treated with an experimental drug versus controls. Nargenicin had a profound effect on DNA synthesis resulting in 60% and >95% reduction in [³H]-uracil incorporation when used to treat Mtb at 2× and 20× MIC, respectively. In contrast, nargenicin had a limited impact on RNA, protein, peptidoglycan, and fatty acid synthesis (Figure 2D). Together, these results were consistent with the replicative polymerase, DnaE1, as the likely target of nargenicin in mycobacteria.

To investigate this further, we assessed the impact of modulating the level of dnaE1 expression on the susceptibility of mycobacteria to nargenicin. We generated a set of fluorescently labeled Mtb hypomorphs carrying inducible dnaE1 CRISPR interference (CRISPRi)⁴⁰ constructs and determined the inhibitory activity of nargenicin against these strains in the presence or absence of the anhydrotetracycline (ATc) inducer. Marked hypersensitization to nargenicin was observed for all four hypomorphs under conditions of dnaE1 silencing (+ATc) but not in the uninduced controls (-ATc) (Figure 3A–C). Importantly, the effect was specific to nargenicin, as evidenced by the lack of effect of dnaE1 silencing on the susceptibility of Mtb to isoniazid or ciprofloxacin, which target mycolic acid biosynthesis and DNA gyrase, respectively (Figure 3C). Together, these results identified DnaE1 as a potential target of nargenicin in Mtb. Using a vector shown previously to conditionally overexpress Msm DnaE1,⁴¹ we found that conditional overexpression of Msm dnaE1 in Msm or Mtb, as further confirmed by quantitative real-time polymerase chain reaction (qRT-PCR) analysis (Figure S4C), had no effect on the nargenicin susceptibility of either organism (Figure S4A,B). Therefore, the DnaE1 copy number alone did not determine nargenicin efficacy in mycobacteria.

Figure 3.

Transcriptional silencing of dnaE1 by inducible CRISPRi selectively hypersensitizes Mtb to nargenicin. (A) Location of sgRNAs 3, 6, 11, and 13 on the Mtb dnaE1 gene (not drawn to scale). (B) In vitro growth phenotypes of the four inducible CRISPRi hypomorphs in dnaE1 constructed in a strain of Mtb carrying a constitutively expressed mScarlet reporter. Strain growth was measured using a microplate alamarBlue assay after 7 days’ exposure to ATc at a concentration ranging from 0.1–200 ng/mL. Columns highlighted in red represent the IC₅₀ for ATc. Data plotted represent the average and standard deviation of two technical replicates for one of the two independent experiments. (C) The four dnaE1 hypomorphs were tested for susceptibility to nargenicin (NRG) alongside the control drugs, ciprofloxacin (CIP) and isoniazid (INH). Drug-mediated growth inhibition of the Mtb dnaE1 mScarlet sgRNA 3 (black), Mtb dnaE1 mScarlet 6 (green), Mtb dnaE1 mScarlet sgRNA 11 (blue), Mtb dnaE1 mScarlet sgRNA 13 (purple) hypomorphs and Mtb mScarlet vector control (red) strains in the presence (+ATc, 100 ng/mL) or absence of an inducer (-ATc) was determined by measuring fluorescence intensity at day 14. Data represent the average and standard error of two technical replicates for one representative experiment, fitted with a dose–response curve (nonlinear regression model). Experiments were performed in triplicate.

Nargenicin Differentially Inhibits Bacterial Polymerases

Based on the microbiological evidence, we investigated whether nargenicin inhibited the DNA polymerase activity of Mtb DnaE1 in a biochemical assay. For comparison, we included S. aureus DnaE, as well as the extensively characterized replicative DNA polymerase from Escherichia coli, DNA polymerase III α (Pol IIIα). To monitor the polymerase activity, we used a real-time polymerase assay in which the incorporation of dGMPs in the primer strand quenches the fluorescent signal of a fluorescein group at the 5′ end of the template strand.⁴¹ We found that nargenicin also inhibits the activity of Mtb DnaE1, albeit at ∼20-fold higher concentrations than S. aureus DnaE (IC₅₀ = 125 and 6 nM, respectively) under the conditions of this assay (Figure 4A). Surprisingly, the E. coli polymerase was only significantly inhibited by nargenicin at concentrations higher than 10 μM.

Figure 4.

Mechanism of DNA polymerase inhibition by nargenicin. (A) Nargenicin inhibition curves of three bacterial replicative DNA polymerases, S. aureus DnaE (green line), Mtb DnaE1 (orange line), and E. coli Pol IIIα (blue line), show IC₅₀ values of 8, 125, and 13 000 nM, respectively. (B) Cryo-EM structure of Mtb DnaE1 bound to DNA and nargenicin in yellow. (C) Close-up view of the nargenicin molecule located between the displaced template base and His787. Cryo-EM map is shown in a blue mesh. (D) Composite binding site of nargenicin between the last base pair of the DNA duplex, the displaced templated base, and the fingers domain of the polymerase. (E) Top view of the binding site showing the “base pairing” of nargenicin onto the last base pair of the DNA duplex (ssDNA overhang not shown for clarity). (F) Nargenicin binding pocket in DnaE1 as viewed from the DNA. All residues located with 5 Å of nargenicin are shown in green sticks. Hydrogen bonds between the protein and nargenicin are indicated with black dashed lines.

Cryo-EM Reveals Mechanism of Inhibition by Nargenicin

To elucidate the mechanism of polymerase inhibition, we determined the structure of full-length Mtb DnaE1 in complex with nargenicin and a DNA substrate by cryo-EM (Figures 4B–F and S5). The structure was determined to a resolution of 2.9 Å with well-defined density for the polymerase active site, DNA, and the bound nargenicin molecule (Figure 4B–F). The cryo-EM structure of Mtb DnaE1 is identical to the previously determined crystal structure⁴² with the exception of the oligonucleotide/oligosaccharide binding (OB) domain that was not included in the crystal structure (Figure S6). The OB-domain is flexible as it shows a weaker density in the cryo-EM map when compared to the rest of the molecule (Figures S5C and S6C). The flexibility of the OB-domain is consistent with cryo-EM structures of E. coli Pol IIIα that show a 70 Å movement of the OB-domain between the DNA-bound and DNA-free state.⁴³

The DNA is bound in a canonical manner between the thumb and fingers domains, as was previously observed for other C-family DNA polymerases.^43,44 The nargenicin molecule is bound in the polymerase active site and is sandwiched between the last base pair of the DNA duplex, the first base of the template strand, and the fingers domain of the polymerase (Figure 4D). Nargenicin occupies both the position of the incoming nucleotide as well as the template base and thus mimics the position of the newly synthesized base pair (Figure 4E). To do so, the first unpaired template base is displaced from its position and bumps into Pro668 of an adjacent helix (residues 668 to 673) that becomes disordered. On the protein side, nargenicin occupies a shallow pocket and only makes three direct contacts with the protein: Arg667 and His787 make a hydrogen bond to two oxygens in nargenicin, while Gln638 makes a hydrogen bond with the nitrogen in the pyrrole ring (Figure 4F). The opposite end of nargenicin that is located on top of His787 makes no interaction with the protein as its nearest neighbor is over 5 Å away.

The binding of nargenicin is reminiscent of the binding of aphidicolin in human DNA polymerase α (hPolα).⁴⁵ Although the two inhibitors differ in the structure (Figure S7A) and the polymerases belong to different families (hPolα is a B-family polymerase, whereas Mtb DnaE1 a C-family polymerase), both inhibitors are bound between the last base pair of the DNA and the polymerase fingers domain, occupy the position of both incoming and templating base, and displace the templating base (Figure S7B,C). However, owing to the structural differences in the polymerase active sites, it is unlikely that nargenicin can inhibit the human polymerase as modeling of nargenicin into the hPolα structure reveals several clashes with the protein (Figure S7D). The similar mechanism of action of the two inhibitors is derived from different organisms—aphidicolin is derived from the mold, Cephalosporium aphidicola,⁴⁵ whereas nargenicin is produced by a Nocardia species^19,20—provides a remarkable example of convergent evolution.

Drug Resistance through Allostery

The structure described above shows that the DNA forms a crucial part of the nargenicin binding site, consistent with the previous observation that binding of nargenicin to S. aureus DnaE only occurs in the presence of DNA.¹⁸ This DNA dependency of binding may also hold the key to the differences in inhibition between S. aureus DnaE, Mtb DnaE1, and E. coli Pol IIIα (Figure 5). The predicted nargenicin binding sites for S. aureus DnaE and E. coli Pol IIIα are highly similar to those of Mtb DnaE1 (Figure 5A,B), and the three residues that make a hydrogen bond with nargenicin are conserved in all three species. Hence, the difference in sensitivity does not appear to have its origin in the binding site. Moreover, a mutation in S. aureus DnaE (a serine to leucine mutation at position 765, equivalent to Mtb DnaE1 residue 860) that renders it resistant to nargenicin is located ∼30 Å away from nargenicin (Figure 5C). This mutation is immediately adjacent to the region of the fingers domain that interacts with the phosphate backbone of the double-stranded DNA substrate. Therefore, we hypothesized that the potency of nargenicin to inhibit a DNA polymerase may be dictated by the polymerase’s affinity for DNA. To test this, we measured the DNA affinity of the three polymerases by fluorescence anisotropy using a primed DNA substrate (Figure 5D). The three DNA polymerases show strikingly different dissociation constants of ∼6 nM for S. aureus DnaE, 250 nM for Mtb DnaE1, and 12 μM for E. coli Pol IIIα. Importantly, these DNA affinities correlate with the relative sensitivities to nargenicin, which follow the same trend (Figure 4A). We also tested the resistant mutation in S. aureus DnaE (S765L), which, as predicted, reduced the affinity for DNA, approximately 14-fold (Figure 5D).

Figure 5.

Sensitivity to nargenicin is dependent on the DNA binding affinity. (A) Nargenicin binding site in a computational model of S. aureus DnaE. The modeled nargenicin is shown in transparent sticks, and the three residues that make a hydrogen bond to nargenicin in Mtb DnaE1 are labeled. The view is identical to Figure 4F. (B) Nargenicin binding site in the crystal structure of E. coli Pol IIIα. The modeled nargenicin is shown in transparent sticks, and the three residues that make a hydrogen bond to nargenicin in Mtb DnaE1 are labeled. The view is identical to Figure 4F. (C) Nargenicin resistance mutation in S. aureus DnaE mapped onto Mtb DnaE1, shown by a magenta sphere, is located 30 Å away from the nargenicin (shown in yellow sticks) but is adjacent to the dsDNA binding region of the polymerase. Residues that interact with the DNA backbone are shown in green sticks. (D) Fluorescence anisotropy DNA binding curves of S. aureus DnaE (green line), Mtb DnaE1 (orange line), and E. coli Pol IIIα (blue line) show dissociation constants of 6 nM, 250 nM, and 12 μM, respectively. S. aureus DnaE^S765L (green dashed line), which carries a mutation that confers antibiotic resistance, shows a dissociation constant of 85 nM, which is ∼14-fold increased, as compared to the wild type.

Taken together, these data support the notion that the potential of nargenicin to inhibit a DNA polymerase is dependent on the polymerase’s affinity for DNA, and any changes which reduce the DNA affinity, lead to reduced nargenicin potency, either through natural variation, as in the case of E. coli Pol IIIα, or through a resistance-conferring mutation,¹⁸ as for S. aureus DnaE. Importantly, S. aureus engages two essential DNA polymerases at the replication fork, namely, PolC and DnaE;⁴⁶ if the activity of one is impaired, the other may compensate. However, mycobacteria rely on only one replicative polymerase, DnaE1. Therefore, nargenicin resistance-conferring mutations in DnaE1 could have catastrophic consequences in mycobacteria, which might explain our inability to isolate spontaneous resistant mutants in Mtb or Msm.

Discussion

We have reported multiple lines of evidence that nargenicin acts as a DNA replication inhibitor in mycobacteria by targeting the essential DnaE1 polymerase, an enzyme identified recently as a highly vulnerable component of the DNA replication machinery in Mtb.⁹ Unlike the commonly used nucleotide analogues that act as chain terminators through the incorporation into the nascent DNA strand, nargenicin does not become incorporated into the DNA. Instead, it is wedged between the terminal base pair of the DNA substrate and the polymerase fingers domain, occupying both the position of the incoming nucleotide and the templating base, which is displaced by nargenicin. This binding mode is analogous to that of the human Pol α inhibitor, aphidicolin, which is derived from the fungus, Cephalosporium aphidicola, and unrelated in structure to nargenicin, indicating that these inhibitors have evolved independently. This unusual mechanism might explain the observation that the antimycobacterial activity of nargenicin was not diminished by overexpression of the cognate target, DnaE1. Based on this mechanism, the DnaE homologue in the Nocardia sp. CS682 producer organism would presumably need to bind nargenicin in a DNA-independent manner to fulfill its postulated “decoy” role in self-resistance.²¹

Nargenicin-mediated disruption of replisome function triggers a physiological response in Mtb, which resembles that elicited by genotoxins, which cause double-stranded breaks (DSBs) (mitomycin C, fluoroquinolones).³⁵ This features upregulation of genes encoding the recombinase involved in recombination repair (recA), the mutasome responsible for DNA-damage-induced mutagenesis and damage tolerance (dnaE2, imuA′, imuB),^35,36 the PafBC-regulated DSB-resecting motor-nuclease (adnAB)^37,47 and a cell wall hydrolase (chiZ),⁴⁸ among other DNA-damage-responsive genes in mycobacteria. The DNA damage response to nargenicin begs the question of whether pharmacological inhibition of DnaE1 by this or other inhibitors might have the unintended consequence of inducing chromosomal mutations, which could fuel the evolution of drug resistance, as documented for sublethal treatment of mycobacteria and other organisms by fluoroquinolones.^49,50 The concomitant downregulation of ftsZ,³⁹sepF,⁵¹whiB2,⁵² and ripA(51) is consistent with cellular elongation, resulting from a block in cell division, followed by cell death. Ablation of the SOS response by deletion of recA, or a key component thereof (mutasome function) by deletion of dnaE2, had no discernible impact on the antimycobacterial activity of nargenicin, suggesting that the LexA/RecA-dependent DNA repair, damage tolerance, and (SOS) mutagenesis systems are unable to rescue mycobacteria from the growth inhibitory effects of nargenicin. Instead, an arrest in cell division, as evidenced by bacillary elongation, appears to precede cell death. However, the DNA damage response to nargenicin also includes genes such as adnA, adnB, cho, and uvrA, which form part of the mycobacterial LexA/RecA-independent regulon controlled by PafBC.^37,53 Given that adnA, adnB, and lhr are among the genes most highly upregulated by nargenicin treatment, it will be important to establish whether, under which conditions, and to what extent the functional disruption of this regulon might have on the susceptibility of mycobacteria to this compound.

Another feature of the nargenicin mode of action was the late, strong signal elicited in the GFP release assay. The induction of chiZ and downregulation of fbpC might be telling in this regard: first, the damage-inducible protein, ChiZ,⁵⁴ has been reported to arrest cell division, increase filamentation, and induce cell lysis when overexpressed.⁴⁸ Second, inactivation of the mycolyltransferase, FbpC, a member of the antigen 85 complex involved in the synthesis of trehalose dimycolate and mycolylarabinogalactan, which are key components of the mycobacterial cell envelope, has been shown to significantly reduce the mycolate content and increase the permeability of the cell envelope to small hydrophobic and hydrophilic molecules.⁵⁵ Thus, in addition to its replication-arresting activity, nargenicin may also compromise the integrity of the mycobacterial outer membrane and thus act as a potentiator of other antitubercular agents whose efficacy is limited by permeation across the mycobacterial cell envelope.

Conclusions

In conclusion, we have shown that nargenicin mediates its bactericidal activity against M. tuberculosis through interaction with DnaE1 in a manner that depends upon the presence of the DNA substrate. In this interaction, the nargenicin molecule wedges itself between DnaE1 and the terminal base pair of the DNA and occupies the place of both the incoming nucleotide and the templating base. By analyzing the physiological consequences of Mtb exposure to nargenicin, we show that the arrest in bacillary replication resulting from the nargenicin-DnaE1 interaction triggers induction of a DNA damage response coupled with an arrest in cell division and an apparent weakening of the mycobacterial cell envelope. In addition to strongly reaffirming the value of natural products as a source of novel antitubercular agents, this work has provided the rationale and platform for focusing target-led drug discovery efforts on a promising new TB drug target.

Methods

Bacterial Strains, Culture Conditions, and Media

The strains used in this study are listed in the key resources table. These include the parental wild-type strains, Mtb H37Rv⁵⁶ and Msm mc²155.⁵⁷ Clinical isolates were obtained from samples collected from new TB cases and retreatment cases of subjects who were enrolled in a prospective longitudinal cohort study (ClinicalTrials.gov identifier, NCT00341601) at the National Masan Tuberculosis Hospital in the Republic of Korea from May 2005 to December 2006.⁵⁸ Mycobacterial strains were cultured in various media depending on the assay. 7H9 OADC was prepared by supplementing Middlebrook 7H9 (Difco) with 10% oleic acid-albumin-dextrose-catalase (OADC) enrichment (Difco), 0.2% glycerol, and either 0.05% Tween-80 (7H9/OADC/Tw) or 0.05% Tyloxapol (7H9/OADC/Tx). 7H9/Glu/ADC/Tw medium was prepared by substituting 10% OADC with 10% albumin-dextrose-catalase (ADC) enrichment (Difco). Similarly, 7H9/Glu/CAS/Tx was prepared by supplementing 7H9 with 0.4% glucose, 0.03% casitone (CAS), 0.081% NaCl, and 0.05% Tx. Glycerol-alanine-salts with iron (GAST-Fe/Tw) medium, pH 6.6, was prepared with 0.03% CAS, 0.005% ferric ammonium citrate, 0.4% dibasic potassium phosphate, 0.2% citric acid, 0.1% l-alanine, 0.12% MgCl₂, 0.06% potassium sulfate, 0.2% ammonium chloride, 0.018% of a 1% sodium hydroxide solution, 1% glycerol, and 0.05% Tween-80. GAST/Tw, an iron limiting media, was prepared as described above but excluding ferric ammonium citrate. All Mtb cultures were incubated at 37 °C in sealed culture flasks with no agitation. The cells were plated onto Middlebrook 7H10 agar plates with a 7H10 agar base (Difco) supplemented with 10% OADC and 0.5% glycerol. Unless indicated otherwise, microbiological assays using the strains described below were performed in 7H9/OADC/Tw media.

The fluorescent reporter strain H37Rv-GFP⁵⁹ and bioluminescent reporter strain PrecA-LUX³³ were grown in media supplemented with kanamycin (Kan) at 20 μg/mL, whereas the Mtb mScarlet strain and Msm ΔL mutant were grown in media supplemented with hygromycin (Hyg) at 50 μg/mL. Mtb and Msm strains carrying the P_UV15-Tet-dnaE1-MYC::L5 vector⁴¹ were grown in media containing Kan at 50 μg/mL and supplemented with ATc at 100 ng/mL to induce expression of dnaE1. The inducible CRISPRi hypomorphs were grown in media containing Kan (25 μg/mL) and Hyg (50 μg/mL) and supplemented with ATc at 100 ng/mL to induce transcriptional silencing. Minimal inhibitory concentrations (MICs) were determined against a range of clinical isolates: Mtb CDC1551;⁶⁰Mtb HN878;⁶¹ drug susceptible isolates, Mtb 0A029, Mtb 0A031 and Mtb 0B229; multi-drug resistant isolates, Mtb 0B123 resistant to isoniazid (INH^R), ofloxacin (OFX^R), para-amino salicylic acid (PAS^R), streptomycin (STR^R), rifampicin (RIF^R); Mtb 0A024 (ethambutol (EMB^R), INH^R, kanamycin (KAN^R), PAS^R, pyrazinamide (PZA^R), STR^R, ethionamide (ETH^R), RIF^R, Mtb 0B026 (EMB^R, INH^R, KAN^R, PAS^R, RIF^R); and an extensively drug resistant strain, Mtb 0B014 (EMB^R, INH^R, KAN^R, OFX^R, PAS^R, RIF^R).⁵⁸

Drug Susceptibility Testing

MIC testing was performed by broth microdilution assay⁵⁹ and quantitatively analyzed with the colorimetric alamarBlue cell viability reagent (Thermo Fischer Scientific), as previously described.³²

Bioluminescence Assay

PrecA-LUX³³ was grown to an OD₆₀₀ of ∼0.4, diluted 10-fold in 7H9/OADC/Tw, and inoculated into white, clear-bottom, 96-well microtiter plates (Greiner CellStar) containing two-fold serial dilutions of the drug. The plates were incubated at 37 °C, and luminescence was recorded every 24 h for 8 days using a SpectraMax i3x plate reader (Molecular Devices). Data were plotted in Prism 9 (GraphPad).

GFP Release Assay

As described previously,³² H37Rv-GFP was grown to an OD₆₀₀ of ∼0.3 in 7H9 OADC and exposed to the drug at 1× or 10× MIC. Every 24 h, over a period of 8 days, 200 μL of culture was harvested, pelleted by centrifugation, and the supernatant was transferred to a black, clear-bottom 96-well microtiter plate (Greiner CellStar) and the fluorescence (excitation, 540 nm; emission, 590 nm) was measured using a SpectraMax i3x plate reader (Molecular Devices). Fluorescence intensity was normalized by OD₆₅₀ and standardized to the value of the drug-free control for each sample.

Time–Kill Kinetics

Mtb was inoculated in the culture medium at an OD₆₀₀ of 0.002, and the drug was added at a concentration of either 1×, 5×, or 10× MIC. Cultures were incubated in sealed culture flasks, and 1 mL aliquot was harvested every 24 h over 8 days. The samples were washed twice in fresh media. One hundred μL aliquots of 10-fold serial dilutions were plated of 7H11 agar, and colony-forming units (CFUs) were enumerated after incubation for 3–4 weeks.

Macromolecular Incorporation Assays

Macromolecular incorporation assays were performed as described.^62,63 Briefly, Mtb cultures were grown to early exponential phase (OD₆₀₀ of ∼0.3) and 1 μCi/mL [³H]-uracil, 2.5 μCi/mL [3H]-phenylalanine, 10 μCi/mL [³H]-N-acetyl glucosamine, and 1 μCi/mL [¹⁴C]-acetate were added to quantify the incorporation of the radiolabeled precursors into either total nucleic acid (i.e., DNA and RNA), protein, cell wall, or fatty acids, respectively. The cells were incubated at 37 °C for 1 h, and 150 μL was transferred to 96-well microtiter plates containing 150 μL of each test compound. Nargenicin was used at 2× and 20× MIC with 1% DMSO included as an untreated control. The specificity of assays was monitored by the inclusion of the pathway-specific antibiotics OFX (5 μg/mL), STR (10 μg/mL), d-cycloserine (DCS, 5 μg/mL), and INH (0.2 μg/mL) as positive controls. The assay plates were incubated at 37 °C for 24 h, and precursor incorporation was terminated by the addition of 300 μL of 20% trichloroacetic acid (TCA). The samples were incubated at 4 °C for 1 h, and the precipitates were collected by vacuum filtration with a 96-well MultiScreen GFC glass fiber plate (Millipore). Precipitates were washed three times with 10% TCA, followed by three 95% ethanol washes, and the plates were allowed to air-dry. Precipitates were resuspended in 50 μL of MicroScint 20 (PerkinElmer), and the radioactivity on each filter was measured in a MicroBeta Liquid Scintillation Counter (PerkinElmer). To distinguish between the incorporation of [³H]-uracil into DNA vs. RNA, the RNA was hydrolyzed with 500 μL of 1 M KOH at 37 °C for 16 h and neutralized with 125 μL of HCl. The samples were then precipitated by adding 625 μL of 20% TCA, and the amount of residual radioactivity present in the DNA precipitates was quantified following filtration and washing as described above. All samples were analyzed in duplicate, and the results represent the percentage of radiolabel incorporation relative to the DMSO-treated control from two independent replicates.

Microscopy

Msm bacilli were imaged to determine their terminal phenotypes under exposure to varying concentrations of antibiotics as previously described.³⁹ Strains were grown to late-log phase (OD₆₀₀ of ∼0.8), filtered once through a Millex syringe filter (5 μm pore size, Millipore), and diluted (1:40) into fresh media. The samples were left untreated, exposed to the carrier (DMSO only) or to the varying concentrations of nargenicin in DMSO (1× MIC, 2× MIC, 4× MIC), and incubated for 18 h at 37 °C while shaking. After exposure, the cultures were spotted on low-melt agarose pads and imaged on a ZEISS Axio Observer using a 100×, 1.4 NA objective with Phase Contrast and Colibri 7 fluorescent illumination system. Images were captured using a Zeiss Axiocam 503. Image processing, cell measurements, and analysis were performed in the FIJI Plugin,⁶⁴ MicrobeJ,⁶⁵ R,⁶⁶ and UMAP, as described.³⁹

Transcriptional Profiling

Microarray experiments and analyses were performed by the NIAID Microarray Research Facility, as previously described,³⁵ including two independent samples for each treatment condition. Datasets from cultures exposed to mitomycin C (0.2 μg/mL) and levofloxacin (10 μg/mL) were compared to nargenicin (129 μg/mL). The top 300 upregulated or downregulated genes, ranked by the average Log 2 fold-change in expression data from two biological repeats, were compared to generate gene shortlists common to all three treatments.

For RNA-seq, qRT-PCR, and microarray experiments, Mtb cultures (20–30 mL) were grown either in roller bottles or culture flasks on a shaker to mid-exponential phase (OD₆₀₀ of ∼0.3–0.5) prior to treatment with nargenicin at 1× or 10× MIC for 6 h. The cells were harvested by centrifugation at 3000g for 10 min and resuspended in 1 mL of Qiazol Lysis Reagent (Qiagen). The cells were lysed with 0.1 mm Zirconia/Silica beads (BioSpec) in a MagNA Lyser Homogenizer (Roche) (6000 rpm, 30 s) three times with 1 min cooling intervals. The samples were centrifuged at 10 000g for 5 min at 4 °C, and the supernatant was transferred into a clean tube containing an equal volume of 100% ethanol. The RNA was purified and treated with DNase on-column using the Direct-zol RNA MiniPrep kit (Zymo Research) according to the manufacturer’s protocol. The samples were eluted in 50 μL of RNase- and DNase-free water. Purified RNA was treated with DNase for an additional 60 min at 37 °C using the TURBO DNA-free kit (Ambion) according to the manufacturer’s protocol. In preparation for microarray analysis and RNA-seq, the sample quality was confirmed using a Bioanalyzer RNA 6000 Nano Kit and Chips (Agilent). For RNA-seq experiments, three independent biological replicates of both nargenicin-treated (10× MIC) and untreated samples were performed. Library preparation and sequencing were done by Admera Health (NJ) using the Illumina NovaSeq S4 sequencing platform. The sequencing strategy included an average of 60 million 150 bp paired-end reads per sample. Reads were demultiplexed to generate raw fastq files for each sample and data were deposited in the NCBI SRA repository (PRJNA722614). Initial quality control (QC) of the raw fastQ files was performed using FastQC.⁶⁷ Reads were trimmed and adapters were removed using Trim Galore. Further QC was done by aligning reads using BWA to the reference genome of Mtb H37Rv, ASM19595v2, GenBank assembly accession no. GCA_000195955.2 (https://www.ncbi.nlm.nih.gov/assembly/GCF_000195955.2), running RSeQC⁶⁸ and dupRadar,⁶⁹ and an amalgamated report generated using MultiQC.⁷⁰ Transcript quantification was performed using Salmon in a mapping-based mode.⁷¹ Normalization and differential expression analysis were done using DESeq. 2⁷² with count normalization by DESeq. 2’s median or ratios. P-values were adjusted for multiple testing using the Benjamini–Hochberg approach, and genes that displayed an absolute Log 2 fold-change >1 and an adjusted p-value <0.05 were considered differentially expressed. Data were visualized in R, and the functional enrichment of upregulated and downregulated shortlists as compared to the full genome was performed in STRING⁷³ using Gene Ontologies, STRING local network clusters, annotated keywords, KEGG pathways, and InterPro protein domains and features as categories. Multiple comparisons were compensated for using the false discovery rate (FDR), with significant enrichment considered as FDR > 0.05.

For qRT-PCR experiments, following TURBO DNase treatment, 250 ng of the RNA was converted to cDNA using SuperScript IV Reverse Transcriptase (Thermo Fischer Scientific). Regions of interest were amplified using primer pairs described in Table S3 and Power SYBR Green PCR master mix (Thermo Fischer Scientific), and transcript levels for three independent samples were quantified on a PikoReal real-time PCR system (Thermo Fischer Scientific). Transcript levels of target genes were normalized to sigA.

Construction of Fluorescent dnaE1 Hypomorphs

The ATc-regulated CRISPRi system developed by Rock et al.⁴⁰ was used to construct inducible dnaE1-targeting Mtb hypomorphs carrying the mScarlet fluorescence reporter.⁷⁴ Briefly, two oligonucleotides complementary to the dnaE1-targeting sequence (Table S3) were annealed and cloned in pLJR965, and the presence of the sgRNA was confirmed by Sanger sequencing. The sequence-verified constructs were electroporated into Mtb mScarlet, selecting on media supplemented with Kan (25 μg/mL) and Hyg (50 μg/mL).

Drug Susceptibility Testing Using Hypomorphs

To assess the impact of dnaE1 silencing on drug susceptibility, the hypomorphs and vector control strains were grown to an OD₆₀₀ of 1.0 and diluted to an OD₆₀₀ of 0.01 in media either with ATc (200 ng/mL) or without the inducer. Fifty μL of the diluted culture was inoculated into each well of a MIC plate containing 50 μL of media with 2-fold dilutions of the drug. Microtiter plates were incubated at 37 °C for 14 days, and the fluorescence (594 nm, excitation; and 569 nm, emission) was recorded using a Spectramax i3x plate reader. Each strain was normalized to the no-drug control to determine the percentage growth inhibition as a function of drug concentration. Dose–response curves were plotted in Prism 9 (GraphPad).

Protein Expression and Purification

Mtb DnaE1 was expressed in Msm and purified as previously described.⁴¹S. aureus DnaE and E. coli Pol IIIα were expressed in E. coli BL21 and purified as previously described.^18,75

DNA Polymerase Assay

DNA polymerase activity was measured using a real-time polymerase assay as described previously.⁴¹ Briefly, reactions were performed using 5 nM DNA polymerase, 10 nM fluorescently labeled DNA substrate (Primer: 5′-TAGGACGAAGGACTCCCAACTTTAGGTGCG, Template: 6-FAM-5′-CCCCCCCCCATGCATGCGCACCTAAAGTTGGGAGTCCTTCGTCCTA), and 100 nM unlabeled DNA substrate (same sequence as above). Reactions contained 100 μM each dNTP, 5 mM MgSO₄, 50 mM HEPES pH 7.5, 100 mM potassium glutamate, 2 mM DTT, 0.5 mg/mL BSA, and 10 nM–10 μM nargenicin, diluted from a stock of 10 mM in 100% DMSO. Then, 10 μL reactions were measured for 20 min at 24 °C in a 384-well plate using a Clariostar plate reader (BMG LABTECH) with excitation and emission filters at 485 and 520 nm, respectively.

Fluorescence Anisotropy

DNA binding was measured using a 5 nM Cy3-labeled DNA substrate (Primer: Cy3-5′-GGTAACGCCAGGGTTTTCCCAGTC3, Template 5′-CGCTCACTGGCCGTCGTTTTACAACGTCGTGACTGGGAAAACCCTGGCGTTACC) and 1 nM–40 μM DNA polymerase. Reaction conditions contained 25 mM HEPES (pH 7.5), 50 mM potassium glutamate, 2 mM DTT, and 0.5 mg/mL BSA. Then, 10 μL reactions were measured at 24 °C in a 384-well plate using a Clariostar plate reader with excitation and emission filters at 540 and 590 nm, respectively.

Cryo-EM Sample Preparation and Imaging

Purified Mtb DnaE1 was diluted to 4 μM in 20 mM PIPES (pH 7.0), 50 mM potassium glutamate, 5 mM MgCl₂, 2 mM DTT, and 0.01% Tween-20. The diluted protein was incubated for 5 min with 10 μM nargenicin (diluted from a stock of 10 mM in 100% DMSO) and 20 μM DNA substrate (Template: 5′- GATAGAGCAGAAGGACGAAGGACTCCCAACTTTAGGTG, Primer: 5′-GCACCTAAAGTTGGGAGTCCTTCGTCCT*T, where the asterisk marks the position of a phosphorothioate bond). Then, 3 μL of sample were adsorbed onto glow-discharged copper R2/1 holey carbon grids (Quantifoil). Grids were glow discharged for 45 s at 25 mA using an EMITECH K950 apparatus. Grids were blotted for one second at ∼80% humidity at 4 °C and flash-frozen in liquid ethane using a Leica EM GP plunge freezer. The grids were loaded into a Titan Krios (FEI) electron microscope operating at 300 kV with a Gatan K3 detector. The slit width of the energy filter was set to 20 eV. Images were recorded with EPU software (Thermo Fisher Scientific) in the counting mode. Dose, magnification, and pixel size are detailed in Table 1.

Table 1. Cryo-EM Data Collection, Refinement, and Validation Statistics.

data collection and processing		model comparison
magnification	×105 000	nonhydrogen atoms	8990
voltage (kV)	300	protein residues	1070
electron exposure e-/Å2	54	B factors (Å2)
defocus range (μm)	0.8–2.0	protein	21–306
pixel size (Å)	0.859	r.m.s deviations
symmetry imposed	C1	bond lengths (Å2)	0.0126
initial particle images (no)	2000000	bond angles (°)	1.1569
final particle images (no)	196709	validation
map resolution (Å)	2.8	MolProbity score	1.47
FSC threshold	0.143	clashscore	4.22
map resolution range (Å)	2.8 to > 5.5	poor rotamers (%)	1.28

refinement		Ramachandran plot
initial model used	5LEW	favored (%)	96.90
model resolution (Å)	2.9	allowed (%)	3.10
FSC threshold	0.143	disallowed (%)	0
map sharpening B-factor (Å2)	–50

Cryo-EM Image Processing

All image processing was performed using RELION 3.1.⁷⁶ The images were drift corrected using RELION’s own (CPU-based) implementation of the UCSF motioncor2, and defocus was estimated using gCTF.⁷⁷ LoG-based auto-picking was performed on all micrographs, and picked particles were 2D classified. After three rounds of 2D classification, classes with different orientations were selected for initial model generation in RELION. The initial model was used as a reference for 3D classification into different classes. The selected classes from 3D classification were subjected to 3D auto refinement followed by different rounds of CTF refinement plus a final round of Bayesian polishing. Polished particles were used for the 3D auto-refine job, and the final map was postprocessed to correct for the modulation transfer function of the detector and sharpened by applying a negative B-factor manually set to −50. A soft mask was applied during postprocessing to generate FSC curves to produce a map of an average resolution of 2.9 Å. The RELION postprocessed map was used to generate improved-resolution EM maps using the SuperEM method,⁷⁸ which aided in model building and refinement. Model building was performed using Coot,⁷⁹ REFMAC5,⁸⁰ the CCPEM-suite,⁸¹ and Phenix.⁸² Details on model refinement and validation are shown in Table 1. In brief, model building started by the rigid-body fitting of the known DnaE1 crystal structure (PDB 5LEW)⁴² into the experimental density map using Coot. The DNA molecule was generated, and the rigid body was fitted into the experimental density map using Coot. Next, we carried out one round of refinement in REFMAC5 using jelly-body restraints, and the model was further manually adjusted in Coot. Final refinement and model validation were performed using Phenix.

Quantification and Statistical Analysis

Statistical details are given in the Methods sections and figure legends, and these include details of the experiments, numbers of replicates (technical and/or experimental), statistical software used, and thresholds of significance. Significance was generally determined as p<0.05, and correction for multiple comparisons was performed, as appropriate. Independent experiments were performed a minimum of two times, and these data were utilized for the generation of summary statistics (mean and standard deviation). Replicate data are included within each figure, as indicated in figure legends, else data are described as a representative experiment. In addition, DNA polymerase assays and DNA binding experiments were performed in three or more independent experiments. Data were not excluded from experimental datasets prior to or during analyses other than during cryo-EM data processing, where particles that did not possess high-resolution features were removed following standard procedures for cryo-EM structure determination.

Glossary

Abbreviations Used

ATc

anhydrotetracycline

cryo-EM

cryo-electron microscopy

DSB

double-stranded breaks

GFP

green fluorescent protein

MDR

multidrug resistant

MIC

minimum inhibitory concentration

Msm

Mycobacterium smegmatis

Mtb

Mycobacterium tuberculosis

OB

oligonucleotide/oligosaccharide binding

Pol IIIα

DNA polymerase III α

TB

tuberculosis

TBDA

Tuberculosis Drug Accelerator

Supporting Information Available

The Supporting Information is available free of charge at https://pubs.acs.org/doi/10.1021/acsinfecdis.1c00643.

• Comparison of the transcriptional response of Mtb to nargenicin versus other genotoxins; binding of aphidicolin in human Pol α; antimycobacterial activity of nargenicin; primers and other oligonucleotides (figures and tables) (PDF)

• Dataset S1 comprises output gene lists of RNA-seq differential gene expression analysis and STRING functional analysis of significantly differentially expressed genes (Data S1); related to Figure 2 and C (XLSX)

Accession Codes

NCBI Sequence Read Archive (SRA) repository (PRJNA722614).

Author Present Address

^# Department of Biochemistry and Microbiology, Rhodes University, Grahamstown 6139, South Africa

Author Contributions

^∇ M.D.C. and M.K.M. contributed equally to this paper. M.D.C. and M.K.M. performed the microbiological profiling and RNA-seq experiments and analyses; G.L.A. and H.I.M.B. performed the DNA microarray and macromolecular incorporation assays; R.T. performed the polymerase assays; A.B. and M.H.L. performed the cryo-EM; J.A. provided bioinformatics support; and S.L. and Y.-M.A. provided technical support. The experiments were designed and the data were analyzed by M.D.C., M.K.M., G.L.A., B.M.C., D.B.O., D.F.W., C.E.B.III, H.I.M.B., M.H.L., and V.M. This manuscript was written by M.D.C., M.K.M., M.H.L., and V.M., and all authors read and edited it. M.H.L., D.B.O., C.E.B.III, and V.M. were Team Leads.

The authors declare the following competing financial interest(s): B.M.C, K.Y. and D.B.O. are employees of Merck Sharp & Dohme Corp., a subsidiary of Merck & Co., Inc., Kenilworth, NJ, USA. C.E.B.III and V.M. are members of the Editorial Advisory Board of ACS Infectious Diseases.

Notes

Plasmids and bacterial strains generated for this study are available upon request.

Notes

RNA-seq datasets from this study are deposited in the NCBI Sequence Read Archive (SRA) repository (PRJNA722614) and are publicly available as of the date of publication. Atomic models and cryo-EM maps have been deposited to the Protein Data Bank and the Electron Microscopy Database under accession codes PDB 7PU7 and EMD 13654. The paper does not report the original code. The pipeline for RNA-seq analysis can be found at the GitHub repository (https://github.com/jambler24/bacterial_transcriptomics). Microscopy data are available from the lead contact upon request. Any additional information required to reanalyze the data reported in this paper is available from the lead contact upon request.