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. 2022 Apr 5;11:e75424. doi: 10.7554/eLife.75424

Listeria monocytogenes requires cellular respiration for NAD+ regeneration and pathogenesis

Rafael Rivera-Lugo 1,†, David Deng 1,†, Andrea Anaya-Sanchez 2, Sara Tejedor-Sanz 3,4, Eugene Tang 1, Valeria M Reyes Ruiz 5,6, Hans B Smith 7, Denis V Titov 1,8,9, John-Demian Sauer 7, Eric P Skaar 5,6, Caroline M Ajo-Franklin 3,4, Daniel A Portnoy 1,10, Samuel H Light 11,12,✉
Editors: Sophie Helaine13, Gisela Storz14
PMCID: PMC9094743  PMID: 35380108

Abstract

Cellular respiration is essential for multiple bacterial pathogens and a validated antibiotic target. In addition to driving oxidative phosphorylation, bacterial respiration has a variety of ancillary functions that obscure its contribution to pathogenesis. We find here that the intracellular pathogen Listeria monocytogenes encodes two respiratory pathways which are partially functionally redundant and indispensable for pathogenesis. Loss of respiration decreased NAD+ regeneration, but this could be specifically reversed by heterologous expression of a water-forming NADH oxidase (NOX). NOX expression fully rescued intracellular growth defects and increased L. monocytogenes loads >1000-fold in a mouse infection model. Consistent with NAD+ regeneration maintaining L. monocytogenes viability and enabling immune evasion, a respiration-deficient strain exhibited elevated bacteriolysis within the host cytosol and NOX expression rescued this phenotype. These studies show that NAD+ regeneration represents a major role of L. monocytogenes respiration and highlight the nuanced relationship between bacterial metabolism, physiology, and pathogenesis.

Research organism: Other

eLife digest

Cellular respiration is one of the main ways organisms make energy. It works by linking the oxidation of an electron donor (like sugar) to the reduction of an electron acceptor (like oxygen). Electrons pass between the two molecules along what is known as an ‘electron transport chain’. This process generates a force that powers the production of adenosine triphosphate (ATP), a molecule that cells use to store energy.

Respiration is a common way for cells to replenish their energy stores, but it is not the only way. A simpler process that does not require a separate electron acceptor or an electron transport chain is called fermentation. Many bacteria have the capacity to perform both respiration and fermentation and do so in a context-dependent manner.

Research has shown that respiration can contribute to bacterial diseases, like tuberculosis and listeriosis (a disease caused by the foodborne pathogen Listeria monocytogenes). Indeed, some antibiotics even target bacterial respiration. Despite being often discussed in the context of generating ATP, respiration is also important for many other cellular processes, including maintaining the balance of reduced and oxidized nicotinamide adenine dinucleotide (NAD) cofactors. Because of these multiple functions, the exact role respiration plays in disease is unknown.

To find out more, Rivera-Lugo, Deng et al. developed strains of the bacterial pathogen Listeria monocytogenes that lacked some of the genes used in respiration. The resulting bacteria were still able to produce energy, but they became much worse at infecting mammalian cells. The use of a genetic tool that restored the balance of reduced and oxidized NAD cofactors revived the ability of respiration-deficient L. monocytogenes to infect mammalian cells, indicating that this balance is what the bacterium requires to infect.

Research into respiration tends to focus on its role in generating ATP. But these results show that for some bacteria, this might not be the most important part of the process. Understanding the other roles of respiration could change the way that researchers develop antibacterial drugs in the future. This in turn could help with the growing problem of antibiotic resistance.

Introduction

Distinct metabolic strategies allow microbes to extract energy from diverse surroundings and colonize nearly every part of the earth. Microbial energy metabolisms vary greatly but can be generally categorized as possessing fermentative or respiratory properties. Cellular respiration is classically described by a multistep process that initiates with the enzymatic oxidation of organic matter and the accompanying reduction of NAD+ (nicotinamide adenine dinucleotide) to NADH. Respiration of fermentable sugars typically starts with glycolysis, which generates pyruvate and NADH. Pyruvate then enters the tricarboxylic acid (TCA) cycle, where its oxidation to carbon dioxide is coupled to the production of additional NADH. NADH generated by glycolysis and the TCA cycle is then oxidized by NADH dehydrogenase to regenerate NAD+ and the resulting electrons are transferred via an electron transport chain to a terminal electron acceptor.

While mammals strictly use oxygen as a respiratory electron acceptor, microbes reside in diverse oxygen-limited environments and have varying and diverse capabilities to use disparate non-oxygen respiratory electron acceptors. Whatever the electron acceptor, electron transfer in the electron transport chain is often coupled to proton pumping across the bacterial inner membrane. This generates a proton gradient or proton motive force, which powers a variety of processes, including ATP production by ATP synthase.

Respiratory pathways are important for several aspects of bacterial physiology. Respiration’s role in establishing the proton motive force allows bacteria to generate ATP from non-fermentable energy sources (which are not amenable to ATP production by substrate-level phosphorylation) and increases ATP yields from fermentable energy sources. In addition to these roles in ATP production, respiratory electron transport chains are directly involved in many other aspects of bacterial physiology, including the regulation of cytosolic pH, transmembrane solute transport, ferredoxin-dependent metabolisms, protein secretion, protein folding, disulfide formation, and flagellar motility (Bader et al., 1999; Driessen et al., 2000; Driessen and Nouwen, 2008; Manson et al., 1977; Slonczewski et al., 2009; Driessen et al., 2000; Tremblay et al., 2013; Wilharm et al., 2004). Beyond the proton motive force, respiration functions to regenerate NAD+, which is essential for enabling the continued function of glycolysis and other metabolic processes. By obviating fermentative mechanisms of NAD+ regeneration, respiration increases metabolic flexibility, which, among other metabolic consequences, can enhance ATP production by substrate-level phosphorylation (Hunt et al., 2010).

Bacterial pathogens reside within a host where they must employ fermentative or respiratory metabolisms to power growth. Pathogen respiratory processes have been linked to host-pathogen conflict in several contexts. Phagocytic cells target bacteria by producing reactive nitrogen species that inhibit aerobic respiration (Richardson et al., 2008). Aggregatibacter actinomycetemcomitans, Salmonella enterica, Streptococcus agalactiae, and Staphylococcus aureus mutants with impaired aerobic respiration are attenuated in murine models of systemic disease (Craig et al., 2013; Hammer et al., 2013; Jones-Carson et al., 2016; Lencina et al., 2018; Lewin et al., 2019; Rivera-Chávez et al., 2016). Aerobic respiration is vital for Mycobacterium tuberculosis pathogenesis and persister cell survival, making respiratory systems validated anti-tuberculosis drug targets (Cook et al., 2014; Hasenoehrl et al., 2020). Respiratory processes that use oxygen, tetrathionate, and nitrate as electron acceptors are important for the growth of S. enterica and Escherichia coli in the mammalian intestinal lumen (Rivera-Chávez et al., 2016; Winter et al., 2010; Winter et al., 2013). While several studies have linked respiration in bacterial pathogens to the use of specific electron donors (i.e. non-fermentable energy sources) within the intestinal lumen, the particular respiratory functions important for systemic bacterial infections remain largely unexplained (Ali et al., 2014; Faber et al., 2017; Gillis et al., 2018; Spiga et al., 2017; Thiennimitr et al., 2011).

Listeria monocytogenes is a human pathogen that, after being ingested on contaminated food, can gain access to the host cell cytosol and use actin-based motility to spread from cell to cell (Freitag et al., 2009). L. monocytogenes has two respiratory-like electron transport chains. One electron transport chain is dedicated to aerobic respiration and uses a menaquinone intermediate and QoxAB (aa3) or CydAB (bd) cytochrome oxidases for terminal electron transfer to O2 (Figure 1A; Corbett et al., 2017). We recently identified a second flavin-based electron transport chain that transfers electrons to extracytosolic acceptors (including ferric iron and fumarate) via a putative demethylmenaquinone intermediate and can promote growth in anaerobic conditions (Figure 1A; Light et al., 2018; Light et al., 2019; Zeng et al., 2021). Final electron transfer steps in this flavin-based electron transport mechanism are catalyzed by PplA and FrdA, which are post-translationally linked to an essential cofactor by the flavin mononucleotide transferase (FmnB) (Light et al., 2018; Méheust et al., 2021).

Figure 1. Respiration impacts L. monocytogenes growth and fermentative output.

(A) Proposed respiratory electron transport chains in L. monocytogenes. Different NADH dehydrogenases likely transfer electrons to distinct but presently unidentified quinones (Qa and Qb). FmnB catalyzes assembly of essential components of the electron transport chain, PplA and FrdA, that can transfer electrons to ferric iron and fumarate, respectively. Other proteins involved in the terminal electron transfer steps are noted. (B) Optical density of L. monocytogenes strains aerobically grown in nutrient-rich media, with the anaerobically grown wildtype strain provided for context. The means and standard deviations from three independent experiments are shown. (C) Fermentation products of L. monocytogenes strains grown to stationary phase in nutrient-rich media under aerobic and anaerobic conditions. Error bars show standard deviations. Results from three independent experiments are shown. (D) Proposed pathways for L. monocytogenes sugar metabolism. The predicted number of NADH generated (+) or consumed (−) in each step is indicated. PplA, peptide pheromone-encoding lipoprotein A; FrdA, fumarate reductase; ΔQC, ΔqoxA/ΔcydAB; ΔQC/fmnB, ΔqoxA/ΔcydAB/fmnB::tn; GLC, glucose; Ack, acetate kinase; Pdh, pyruvate dehydrogenase; Pfl, pyruvate formate-lyase; DMK, demethylmenaquinone.

Figure 1—source data 1. Source data for Figure 1B.
Figure 1—source data 2. Source data for Figure 1C.

Figure 1.

Figure 1—figure supplement 1. Use of respiratory electron acceptors enhances Listeria monocytogenes growth in nutrient-rich media.

Figure 1—figure supplement 1.

(A) Optical density of L. monocytogenes strains grown anaerobically in nutrient-rich media. The data represent the means and standard deviations from three independent experiments. (B) Optical density of anaerobically grown strains in nutrient-rich media supplemented with the alternative electron acceptors ferric iron (Fe3+) or fumarate (fum), as indicated. The means and standard deviations from three independent experiments are shown.
Figure 1—figure supplement 1—source data 1. Source data for Figure 1—figure supplement 1A.
Figure 1—figure supplement 1—source data 2. Source data for Figure 1—figure supplement 1B.
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L. monocytogenes resembles fermentative microbes in lacking a functional TCA cycle (Trivett and Meyer, 1971). Despite thus being unable to completely oxidize sugar substrates, previous studies have shown that aerobic respiration is important for the systemic spread of L. monocytogenes (Chen et al., 2017; Corbett et al., 2017; Stritzker et al., 2004). Microbes that similarly contain a respiratory electron transport chain but lack a TCA cycle are considered to employ a respiro-fermentative metabolism (Pedersen et al., 2012). Respiro-fermentative metabolisms tune the cell’s fermentative output and often manifest with the respiratory regeneration of NAD+ enabling a shift from the production of reduced (e.g. lactic acid and ethanol) to oxidized (e.g. acetic acid) fermentation products. In respiro-fermentative lactic acid bacteria closely related to L. monocytogenes, cellular respiration results in a modest growth enhancement, but is generally dispensable (Duwat et al., 2001; Pedersen et al., 2012).

The studies presented here sought to address the role of respiration in L. monocytogenes pathogenesis. Our results confirm that L. monocytogenes exhibits a respiro-fermentative metabolism and show that its two respiratory systems are partially functionally redundant under aerobic conditions. We find that the respiration-deficient L. monocytogenes strains exhibit severely attenuated virulence and lyse within the cytosol of infected cells. Finally, we selectively abrogate the effect of diminished NAD+ regeneration in respiration-deficient L. monocytogenes strains by heterologous expression of a water-forming NADH oxidase (NOX) and find that this restores virulence. These results thus elucidate the basis of L. monocytogenes cellular respiration and demonstrate that NAD+ regeneration represents a key function of this activity in L. monocytogenes pathogenesis.

Results

L. monocytogenes’ electron transport chains have distinct roles in aerobic and anaerobic growth

We selected previously characterized ΔqoxA/ΔcydAB (ΔQC) and ΔfmnB L. monocytogenes strains to study the role of aerobic respiration and extracellular electron transfer, respectively (Chen et al., 2017; Light et al., 2018). In addition, we generated a ΔqoxA/ΔcydAB/fmnB::tn (ΔQC/fmnB) L. monocytogenes strain to test for functional redundancies of aerobic respiration and extracellular electron transfer. Initial studies measured the growth of these strains on nutritionally rich brain heart infusion (BHI) media in the presence/absence of electron acceptors.

Compared to anaerobic conditions that lacked an electron acceptor, we found that aeration led to a relatively modest increase in growth of wildtype and ΔfmnB strains (Figure 1B and Figure 1—figure supplement 1a). This growth enhancement could be attributed to aerobic respiration, as aerobic growth of the ΔQC strain resembled anaerobically cultured strains (Figure 1B and Figure 1—figure supplement 1a). Similarly, in anaerobic conditions, inclusion of the extracellular electron acceptors, ferric iron and fumarate, resulted in a small growth enhancement of wildtype L. monocytogenes (Figure 1—figure supplement 1b). This phenotype could be attributed to extracellular electron transfer, as ferric iron or fumarate failed to stimulate growth of the ΔfmnB strain (Figure 1—figure supplement 1b). These findings are consistent with aerobic respiration and extracellular electron transfer possessing distinct roles in aerobic and anaerobic environments, respectively.

The ΔQC/fmnB strain exhibited the most striking growth pattern. This strain lacked a phenotype under anaerobic conditions but had impaired aerobic growth, even relative to the ΔQC strain (Figure 1B). Notably, ΔQC/fmnB was the sole strain tested with a substantially reduced growth rate in the presence of oxygen (Figure 1B). These observations suggest that aerobic extracellular electron transfer activity can partially compensate for the loss of aerobic respiration and that oxygen inhibits L. monocytogenes growth in the absence of both electron transport chains.

Respiration alters L. monocytogenes’ fermentative output

Respiration is classically defined by the complete oxidation of an electron donor (e.g. glucose) to carbon dioxide in the TCA cycle. However, L. monocytogenes lacks a TCA cycle and instead converts sugars into multiple fermentation products (Romick et al., 1996). We thus asked how respiration impacts L. monocytogenes’ fermentative output. Under anaerobic conditions that lacked an alternative electron acceptor, L. monocytogenes exhibited a pattern of mixed acid fermentation, with lactic acid being most abundant and ethanol, formic acid, and acetic acid being produced at lower levels (Figure 1C). By contrast, under aerobic conditions L. monocytogenes almost exclusively produced acetic acid (Figure 1C). Consistent with respiration being partially responsible for the distinct aerobic vs. anaerobic responses, ΔQC and ΔQC/fmnB strains failed to undergo drastic shifts in fermentative output when grown in aerobic conditions. The ΔQC strain mainly produced lactic acid in the presence of oxygen, and this trend was even more pronounced in the ΔQC/fmnB strain, which almost exclusively produced lactic acid (Figure 1C). These results show that aerobic respiration induces a shift to acetic acid production and support the conclusion that L. monocytogenes’ two electron transport chains are partially functionally redundant in aerobic conditions.

A comparison of fermentative outputs across the experimental conditions also clarifies the basis of central energy metabolism in L. monocytogenes. A classical glycolytic metabolism in L. monocytogenes likely generates ATP and NADH. In the absence of oxygen or an alternative electron acceptor, NAD+ is regenerated by coupling NADH oxidation to the reduction of pyruvate to lactate or ethanol. In the presence of oxygen, NADH oxidation is coupled to the reduction of oxygen, and pyruvate is converted to acetate. Moreover, the pattern of anaerobic formate production is consistent with aerobic acetyl-CoA production through pyruvate dehydrogenase and anaerobic production through pyruvate formate-lyase (Figure 1D). Collectively, these observations suggest that L. monocytogenes prioritizes balancing NAD+/NADH levels in the absence of an electron acceptor and maximizing ATP production in the presence of oxygen. In the absence of oxygen, NAD+/NADH redox homeostasis is achieved by minimizing NADH produced in acetyl-CoA biosynthesis and by consuming NADH in lactate/ethanol fermentation (Figure 1D). In the presence of oxygen, ATP yields are maximized through respiration and increased substrate-level phosphorylation by acetate kinase activity (Figure 1D).

Respiratory capabilities are essential for L. monocytogenes pathogenesis

We next asked about the role of cellular respiration in intracellular L. monocytogenes growth and pathogenesis. The ΔfmnB mutant deficient for extracellular electron transfer was previously shown to resemble the wildtype L. monocytogenes strain in a murine model of infection (Light et al., 2018). We found that this mutant also did not differ from wildtype L. monocytogenes in growth in bone marrow-derived macrophages (BMMs) and a plaque assay that monitors bacterial growth and cell-to-cell spread (Figure 2A and B). Consistent with previous reports, the ΔQC strain deficient for aerobic respiration was attenuated in the plaque assay and murine model of infection, but resembled wildtype L. monocytogenes in macrophage growth (Figure 2A–C; Chen et al., 2017; Corbett et al., 2017). Combining mutations that resulted in the loss of both extracellular electron transfer and aerobic respiration produced even more pronounced phenotypes. The ΔQC/fmnB strain did not grow intracellularly in macrophages and fell below the limit of detection in the plaque assay and murine infection model (Figure 2A–C). Consistent with this phenotype reflecting a loss of respiratory activity, we observed that a mutant that targeted the two respiratory NADH dehydrogenases resulted in a similar phenotype in the plaque assay (Figure 2A). These results thus demonstrate that respiratory activities are essential for L. monocytogenes virulence, and that the organism’s two respiratory pathways are partially functionally redundant within a mammalian host.

Figure 2. Respiration is required for L. monocytogenes virulence.

Figure 2.

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(A) Plaque formation by cell-to-cell spread of L. monocytogenes strains in monolayers of mouse L2 fibroblast cells. The mean plaque size of each strain is shown as a percentage relative to the wildtype plaque size. Error bars represent standard deviations of the mean plaque size from two independent experiments. Statistical analysis was performed using one-way ANOVA and Dunnett’s post-test comparing wildtype to all the other strains. ****, p<0.0001; ns, no significant difference (p>0.05). (B) Intracellular growth of L. monocytogenes strains in murine bone marrow-derived macrophages (BMMs). At 1-hour post-infection, infected BMMs were treated with 50 μg/mL of gentamicin to kill extracellular bacteria. Colony-forming units (CFU) were enumerated at the indicated times. Results are representative of two independent experiments. (C) Bacterial burdens in murine spleens and livers 48 hours post-intravenous infection with indicated L. monocytogenes strains. The median values of the CFUs are denoted by black bars. The dashed lines represent the limit of detection. Data were combined from two independent experiments, n = 10 mice per strain. Statistical significance was evaluated using one-way ANOVA and Dunnett’s post-test using wildtype as the control. ****, p<0.0001. ΔQC, ΔqoxA/ΔcydAB; ΔQC/fmnB, ΔqoxA/ΔcydAB/fmnB::tn; Δndh1/ndh2, Δndh1/ndh2::tn.

Figure 2—source data 1. Source data for Figure 2A.
Figure 2—source data 2. Source data for Figure 2B.
Figure 2—source data 3. Source data for Figure 2C.

Expression of NOX restores NAD+ levels in L. monocytogenes respiration mutants

Cellular respiration both regenerates NAD+ and establishes a proton motive force that is important for various aspects of bacterial physiology. The involvement of respiration in these two distinct processes can confound the analysis of respiration-impaired phenotypes. However, the heterologous expression of water-forming NADH oxidase (NOX) has been used to decouple these functionalities in mammalian cells (Figure 3A; Titov et al., 2016). Because NOX regenerates NAD+ without pumping protons across the membrane, its introduction to a respiration-deficient cell can correct the NAD+/NADH imbalance, thereby isolating the role of the proton motive force in the phenotype (Lopez de Felipe et al., 1998; Titov et al., 2016).

Figure 3. Water-forming NADH oxidase (NOX) restores redox homeostasis in respiration-deficient L. monocytogenes strains.

(A) Reaction catalyzed by the Lactococcus lactis water-forming NOX, which is the same as aerobic respiration without the generation of a proton motive force. (B) NAD+/NADH ratios of parent and NOX-complemented L. monocytogenes strains grown aerobically in nutrient-rich media to mid-logarithmic phase. Results from three independent experiments are presented as means and standard deviations. Statistical significance was calculated using one-way ANOVA and Dunnett’s post-test using the wildtype parent strain as the control. ****, p<0.0001; ***, p<0.001; **, p<0.01; ns, not statistically significant (p>0.05). (C) Fermentation products of L. monocytogenes strains grown in nutrient-rich media under aerobic conditions. Error bars show standard deviations. Results from three independent experiments are shown. ΔQC, ΔqoxA/ΔcydAB; ΔQC/fmnB, ΔqoxA/ΔcydAB/fmnB::tn; + NOX, strains complemented with L. lactis nox.

Figure 3—source data 1. Source data for Figure 3B.
Figure 3—source data 2. Source data for Figure 3C.

Figure 3.

Figure 3—figure supplement 1. NOX expression in respiration-deficient mutants fails to rescue swarming motility.

Figure 3—figure supplement 1.

The swarming motility of parent and NOX-complemented Listeria monocytogenes strains is shown as a percentage relative to the wildtype swarming diameter following 48 hours incubation at 30°C. Error bars represent standard deviations of the mean swarming diameters from three independent experiments. Statistical significance between the wildtype and mutant strains was calculated using one-way ANOVA and unpaired two-tailed t test was utilized to determine significance between parent and NOX-complemented strains. ****, p<0.0001; ***, p<0.001; **, p<0.01; *, p<0.05; ns, no significant difference (p>0.05).
Figure 3—figure supplement 1—source data 1. Source data for Figure 3—figure supplement 1.
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To address which aspect of cellular respiration was important for L. monocytogenes pathogenesis, we introduced the previously characterized Lactococcus lactis water-forming NOX to the genome of respiration-deficient L. monocytogenes strains (Heux et al., 2006; Neves et al., 2002a; Neves et al., 2002b). We confirmed that the ΔQC and ΔQC/fmnB strains exhibited decreased NAD+/NADH levels and that constitutive expression of NOX rescued this phenotype (Figure 3B). Consistent with the altered fermentative output of the ΔQC/fmnB strain resulting from impaired NAD+ regeneration, we observed that NOX expression restored the predominance of acetic acid production to the aerobically grown cells (Figure 3C).

To confirm that NOX expression specifically impacts NAD+/NADH-dependent phenotypes, we tested the effect of NOX expression on bacterial motility. Consistent with respiration impacting flagellar function through the proton motive force, we found that ΔQC/fmnB exhibited impaired bacterial motility and that this phenotype was resilient to NOX expression (Manson et al., 1977; Figure 3—figure supplement 1). These experiments thus provide evidence that NOX expression provides a tool to specifically manipulate the NAD+/NADH ratio in L. monocytogenes.

Respiration is critical for regenerating NAD+ during L. monocytogenes pathogenesis

We next sought to dissect the relative importance of respiration in generating a proton motive force versus maintaining redox homeostasis for L. monocytogenes virulence. We tested NOX-expressing ΔQC and ΔQC/fmnB strains for macrophage growth, plaque formation, and in the murine infection model. Expression of NOX almost fully rescued the plaque and macrophage growth phenotypes of the ΔQC and ΔQC/fmnB strains (Figure 4A and B). NOX expression also partially rescued L. monocytogenes virulence in the murine infection model (Figure 4C). Notably, NOX expression had a greater impact on the L. monocytogenes load in the spleen than the liver, suggesting distinct functions of respiration for L. monocytogenes colonization of these two organs (Figure 4C). These results thus suggest that NAD+ regeneration represents the primary role of respiration in L. monocytogenes pathogenesis to an organ-specific extent.

Figure 4. NOX expression restores virulence to respiration-deficient L. monocytogenes strains.

Figure 4.

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(A) Plaque formation by cell-to-cell spread of L. monocytogenes strains in monolayers of mouse L2 fibroblast cells. The mean plaque size of each strain is shown as a percentage relative to the wildtype plaque size. Error bars represent standard deviations of the mean plaque size from two independent experiments. Statistical analysis was performed using the unpaired two-tailed t test. ****, p<0.0001; ns, no significant difference (p>0.05). (B) Intracellular growth of L. monocytogenes strains in murine bone marrow-derived macrophages (BMMs). At 1-hour post-infection, infected BMMs were treated with 50 μg/mL of gentamicin to kill extracellular bacteria. Colony-forming units (CFU) were enumerated at the indicated times. Results are representative of three independent experiments. (C) Bacterial burdens in murine spleens and livers 48 hours post-intravenous infection with indicated L. monocytogenes strains. The median values of the CFUs are denoted by black bars. The dashed lines represent the limit of detection. Data were combined from two independent experiments, n = 10 mice per strain, but for the wildtype +NOX strain (n = 9 mice). Statistical significance was evaluated using one-way ANOVA and Dunnett’s post-test using the wildtype control strain to compare with the NOX-complemented strains. Significance between the parental and the NOX-complemented strains was determined using the unpaired two-tailed t test. ****, p<0.0001; **, p<0.01; ns, no significant difference (p>0.05). ΔQC, ΔqoxA/ΔcydAB; ΔQC/fmnB, ΔqoxA/ΔcydAB/fmnB::tn; Δndh1/ndh2, Δndh1/ndh2::tn; + NOX, strains complemented with Lactococcus lactis nox.

Figure 4—source data 1. Source data for Figure 4A.
Figure 4—source data 2. Source data for Figure 4B.
Figure 4—source data 3. Source data for Figure 4C.

Impaired redox homeostasis is associated with increased cytosolic L. monocytogenes lysis

We next asked why respiration-mediated redox homeostasis was critical for L. monocytogenes pathogenesis. We reasoned that previous descriptions of L. monocytogenes quinone biosynthesis mutants might provide a clue. Quinones are a family of redox-active cofactors that have essential functions in respiratory electron transport chains (Collins and Jones, 1981). Our previous studies suggested that distinct quinones function in flavin-based electron transfer and aerobic respiration (Light et al., 2018). A separate set of studies found that L. monocytogenes quinone biosynthesis mutants exhibited divergent phenotypes. L. monocytogenes strains defective in upstream steps of the quinone biosynthesis pathway (menB, menC, menD, menE, and menF) exhibited increased bacteriolysis in the cytosol of host cells and were severely attenuated for virulence (Figure 5A). By contrast, L. monocytogenes strains defective in downstream steps of the quinone biosynthesis pathway (menA and menG) did not exhibit increased cytosolic bacteriolysis and had less severe virulence phenotypes (Chen et al., 2019, Chen et al., 2017; Smith et al., 2021; Figure 5A). These divergent phenotypic responses resemble the loss of aerobic respiration versus the loss of aerobic respiration plus flavin-based electron transfer observed in our studies. The distinct virulence phenotype of quinone biosynthesis mutants could thus be explained by the upstream portion of the quinone biosynthesis pathway being required for both aerobic respiration and flavin-based electron transfer, with the downstream portion of the pathway only being required for aerobic respiration (Figure 5A).

Figure 5. Impaired redox homeostasis accounts for elevated bacteriolysis of a respiration-deficient L. monocytogenes strain in the cytosol of infected cells.

Figure 5.

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(A) Proposed L. monocytogenes quinone biosynthesis pathway. Arrows indicate the number of enzymes that catalyze each reaction. An unidentified demethylmenaquinone (DMK) is proposed to be required for the flavin-based electron transfer pathway and MK7 required for aerobic respiration. Loss of the upstream portion of the pathway is anticipated to impact both electron transport chains. (B) Plaque formation by cell-to-cell spread of L. monocytogenes strains in monolayers of mouse L2 fibroblast cells. The mean plaque size of each strain is shown as a percentage relative to the wildtype plaque size. Error bars represent standard deviations of the mean plaque size from two independent experiments. Statistical analysis was performed using the unpaired two-tailed t test. ****, p<0.0001. (C) Bacterial burdens in murine spleens and livers 48 hours post-intravenous infection with indicated L. monocytogenes strains. The median values of the CFUs are denoted by black bars. The dashed lines represent the limit of detection. Data were combined from two independent experiments, n = 10 mice per strain. Statistical significance was evaluated using one-way ANOVA and Dunnett’s post-test using the wildtype strain as the control to compare with the NOX-complemented strain. Significance between the parental and the NOX-complemented strain was determined using the unpaired two-tailed t test. ****, p<0.0001. (D) Bacteriolysis of L. monocytogenes strains in bone marrow-derived macrophages. The data are normalized to wildtype bacteriolysis levels and presented as means and standard deviations from three independent experiments. Statistical significance was calculated using one-way ANOVA and Dunnett’s post-test using the wildtype parent strain as the control. ****, p<0.0001; ns, no significant difference (p>0.05).

Figure 5—source data 1. Source data for Figure 5B.
Figure 5—source data 2. Source data for Figure 5C.
Figure 5—source data 3. Source data for Figure 5D.

Based on the proposed roles of quinones in respiration, we hypothesized that the severe phenotypes previously described for the upstream quinone biosynthesis mutants were due to an imbalance in the NAD+/NADH ratio. To address this hypothesis, we first confirmed that the ΔmenB strain, which is defective in upstream quinone biosynthesis, exhibited a phenotype similar to the ΔQC/fmnB strain for plaque formation and in the murine infection model (Figure 5B and C). We next tested the effect of NOX expression on virulence phenotypes for the ΔmenB strain. NOX expression rescued ΔmenB phenotypes for plaque formation and in the murine infection model to a strikingly similar extent as the ΔQC/fmnB strain (Figure 5B and C). These results thus provide evidence that quinone biosynthesis is essential for respiration and that the severity of the ΔmenB phenotype is largely due to the role of respiration in regenerating NAD+.

Numerous adaptations allow L. monocytogenes to colonize the host cytosol, including resistance to bacteriolysis. Minimizing bacteriolysis within the host cytosol is important to the pathogen because it can activate the host’s innate immune responses, including pyroptosis, a form of programmed cell death, which severely reduces L. monocytogenes virulence (Sauer et al., 2010). L. monocytogenes strains deficient for the upstream quinone biosynthesis steps were previously identified as having an increased susceptibility to bacteriolysis in the macrophage cytosol (Chen et al., 2017). We thus hypothesized that decreased virulence of respiration-deficient strains might relate to increased cytosolic bacteriolysis.

Using a previously described luciferase-based assay to quantify cytosolic plasmid release, we confirmed that the ΔmenB strain exhibited increased intracellular bacteriolysis (Figure 5D; Sauer et al., 2010). We further found that NOX expression rescued ΔmenB bacteriolysis, but not a comparable bacteriolysis phenotype in a ΔglmR strain that was previously shown to result from unrelated deficiencies in cell wall biosynthesis (Figure 5D; Pensinger et al., 2021). These studies thus show that efficient NAD+ regeneration is essential for limiting cytosolic bacteriolysis and suggest a model whereby respiration-mediated NAD+ regeneration promotes virulence, in part, by maintaining cell viability and facilitating evasion of innate immunity (Figure 6).

Figure 6. Model of the role of respiration in L. monocytogenes pathogenesis.

Figure 6.

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On the left, an intracellular bacterium with the ability to oxidize NADH and transfer electrons through the aerobic and extracellular electron transfer electron transport chains can regenerate and maintain high NAD+ levels allowing the bacterium to grow and be virulent. On the right, an intracellular bacterium unable to regenerate NAD+, by lacking the electron transport chains, is avirulent because it lyses in the cytosol of infected cells.

Discussion

Cellular respiration is one of the most fundamental aspects of bacterial metabolism and a validated antibiotic target. Despite its importance, the role of cellular respiration in systemic bacterial pathogenesis has remained largely unexplained. The studies reported here address the basis of respiration in the pathogen L. monocytogenes, identifying two electron transport chains that are partially functionally redundant and essential for pathogenesis. We find that restoring NAD+ regeneration to respiration-deficient L. monocytogenes strains through the heterologous expression of NOX prevents bacteriolysis within the host cytosol and rescues pathogenesis. These findings thus support the conclusion that NAD+ regeneration represents a major role of L. monocytogenes respiration during pathogenesis.

Our results clarify several aspects of the basis and significance of energy metabolism in L. monocytogenes. In particular, our studies establish the relationship between L. monocytogenes’ two electron transport chains – confirming previous observations that flavin-based electron transfer enhances anaerobic L. monocytogenes growth and revealing a novel aerobic function of this pathway (Light et al., 2018; Zeng et al., 2021). While the benefit of flavin-based electron transfer was only apparent in the absence of aerobic respiration, identifying the substrates and functions of aerobic activation of this pathway may provide an interesting avenue for future studies.

Our studies further reveal that L. monocytogenes employs a respiro-fermentative metabolic strategy characterized by production of the reduced fermentation products lactate and ethanol in the absence of an electron acceptor and acetate when a respiratory pathway is activated. This respiro-fermentative metabolism is consistent with the proton motive force being less central to L. monocytogenes energy metabolism and with a primary role of respiration being to unleash ATP production via acetate kinase catalyzed substrate-level phosphorylation (Figure 1D).

The importance of cellular respiration for non-proton motive force-related processes is further supported by observations about the ability of heterologous NOX overexpression to rescue the severe pathogenesis phenotypes of respiration-deficient L. monocytogenes strains. NOX expression fully rescued in vitro growth defects and partially rescued virulence in the mouse model of disease, suggesting that NAD+ regeneration represents the sole function of respiration in some cell types and a major (but not sole) function of respiration in systemic disease. These findings suggest that a presently unaccounted for proton motive force-dependent aspect of microbial physiology is likely important for systemic disease. Considering the significance of cellular respiration as an antibiotic target, these insights into the role respiration be relevant for future drug development strategies.

While our studies provide evidence that NAD+ regeneration is critical for preventing intracellular bacteriolysis, some ambiguity remains regarding the molecular mechanism linking NAD+/NADH imbalance to the loss of L. monocytogenes virulence. One potential clue comes from a recent study of the transcriptional regulator Rex. Rex senses a low NAD+/NADH ratio and derepresses reductive fermentation pathways, including those that produce lactate and ethanol, and a L. monocytogenes strain deficient in Rex exhibited decreased virulence (Halsey et al., 2021). Activation of part of the Rex regulon may at least partially account for the NAD+/NADH-dependent phenotypes observed in our studies. The centrality of NAD+ regeneration to L. monocytogenes also falls in line with relatively recent studies of mammalian respiration. Several studies have shown that the inability of respiration-deficient mammalian cells to regenerate NAD+ impacts anabolic metabolisms and inhibits growth (Birsoy et al., 2015; Li et al., 2020; Sullivan et al., 2015; Titov et al., 2016). Our discovery of a similar role of respiration in a bacterial pathogen thus suggests that the importance of respiration for NAD+ regeneration is a fundamental property conserved across the kingdoms of life.

Materials and methods

Bacterial culture and strains

All strains of L. monocytogenes used in this study were derived from the wildtype 10403S (streptomycin-resistant) strain (see Table 1 for references and additional details). The L. lactis water-forming nox (NCBI accession WP_010905313.1) was cloned into the pPL2 vector downstream of the constitutive Phyper promoter and integrated into the L. monocytogenes genome via conjugation, as previously described (Lauer et al., 2002; Shen and Higgins, 2005). The ΔQC/fmnB strain was generated from ΔQC and fmnB::tn strains using generalized transduction protocols with phage U153, as previously described (Hodgson, 2000; Reniere et al., 2016).

Table 1. Bacterial strains used in this study.

Strains Strain number Reference
Listeria monocytogenes (wildtype) 10403S Bécavin et al., 2014
ΔcydAB/ΔqoxA DP-L6624 Chen et al., 2017
ΔcydAB/ΔqoxA/fmnB::tn DP-L7190 This study
ΔfmnB DP-L7195 This study
Wildtype + pPL2 NOX DP-L7188 This study
ΔcydAB/ΔqoxA + pPL2 NOX DP-L7189 This study
ΔcydAB/ΔqoxA/fmnB::tn + pPL2 NOX DP-L7191 This study
ΔflaA DP-L5986 Nguyen et al., 2020
Δndh1/ndh2::tn DP-L6626 This study
Δndh1/ndh2::tn + pPL2 NOX DP-L7253 This study
Wildtype + pBHE573 JDS18 Sauer et al., 2010
Wildtype + pPL2 NOX + pBHE573 JDS2328 This study
ΔmenB + pBHE573 JDS1191 Chen et al., 2017
ΔmenB + pPL2 NOX + pBHE573 JDS2333 This study
Δhly + pBHE573 JDS19 Sauer et al., 2010
ΔglmR + pBHE573 JDS21 Sauer et al., 2010
ΔglmR + pPL2 NOX + pBHE573 JDS2329 This study
Escherichia coli SM10
pPL2-NOX DP-E7206 This study
pBHE573 JDS17 Sauer et al., 2010
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L. monocytogenes cells were grown at 37°C in filter-sterilized BHI media. Growth curves were spectrophotometrically measured by optical density at a wavelength of 600 nm (OD600). An anaerobic chamber (Coy Laboratory Products) with an environment of 2% H2 balanced in N2 was used for anaerobic experiments. Media was supplemented with 50 mM ferric ammonium citrate or 50 mM fumarate for experiments that addressed the effect of electron acceptors on L. monocytogenes growth.

Plaque assays

L. monocytogenes strains were grown overnight slanted at 30°C and were diluted in sterile phosphate-buffered saline (PBS). Six-well plates containing 1.2 × 106 mouse L2 fibroblast cells per well were infected with the L. monocytogenes strains at a multiplicity of infection (MOI) of approximately 0.1. At 1-hour post-infection, the L2 cells were washed with PBS and overlaid with Dulbecco’s Modified Eagle Medium (DMEM) containing 0.7% agarose and gentamicin (10 µg/mL) to kill extracellular bacteria, and then plates were incubated at 37°C with 5% CO2. At 72-hour post-infection, L2 cells were overlaid with a staining mixture containing DMEM, 0.7% agarose, neutral red (Sigma), and gentamicin (10 µg/mL), and plaques were scanned and analyzed using ImageJ, as previously described (Reniere et al., 2016; Sun et al., 1990).

Intracellular macrophage growth curves

L. monocytogenes strains were grown overnight slanted at 30°C and were diluted in sterile PBS. A total of 3 × 106 BMMs from C57BL/6 mice were seeded in 60 mm non-TC treated dishes containing 14 12 mm glass coverslips in each dish and infected at an MOI of 0.25 as previously described (Portnoy et al., 1988; Reniere et al., 2016).

Mouse virulence experiments

L. monocytogenes strains were grown at 37°C with shaking at 200 r.p.m. to mid-logarithmic phase. Bacteria were collected and washed in PBS and resuspended at a concentration of 5 × 105 colony-forming units (CFU) per 200 μL of sterile PBS. The 8-week-old female CD-1 mice (Charles River) were then injected with 1 × 105 CFU via the tail vein. At 48 hours post-infection, spleens and livers were collected, homogenized, and plated to determine the number of CFU per organ.

NAD+/NADH assay

L. monocytogenes strains were grown at 37°C with shaking at 200 r.p.m. to mid-logarithmic phase. Cultures were centrifuged and then resuspended in PBS. Resuspended bacteria were then lysed by vortexing with 0.1-mm-diameter zirconia–silica beads for 10 min. Lysates were used to measure NAD+ and NADH levels using the NAD/NADH-Glo assay (Promega, G9071) by following the manufacturer’s protocol.

Fermentation product measurements

Organic acids and ethanol were measured by high-performance liquid chromatography (Agilent, 1260 Infinity), using a standard analytical system (Shimadzu, Kyoto, Japan) equipped with an Aminex Organic Acid Analysis column (Bio-Rad, HPX-87H 300 × 7.8 mm) heated at 60°C. The eluent was 5 mM of sulfuric acid, used at a flow rate of 0.6 mL/min. We used a refractive index detector 1260 Infinity II RID and a 1260 Infinity II variable wavelength detector. A five-point calibration curve based on peak area was generated and used to calculate concentrations in the unknown samples.

Motility assay

L. monocytogenes strains were grown overnight slanted at 30°C and were diluted in sterile PBS. Cultures were normalized to an OD600 of 1.0 and 1 μL of cultures were inoculated on semisolid BHI 0.3% agar. Mutant swarming diameters relative to wildtype were quantified following 48 hours incubation at 30°C.

Intracellular bacteriolysis assay

Bacteriolysis assays were performed as previously described (Chen et al., 2017). Briefly, immortalized Ifnar-/- macrophages were plated at a concentration of 5 × 105 cells per well in a 24-well plate. Cultures of L. monocytogenes strains were grown overnight slanted at 30°C and diluted to a final concentration of 5 × 108 CFU per mL. Diluted cultures were then used to infect macrophages at an MOI of 10. At 1-hour post-infection, wells were aspirated, and the media was replaced with media containing 50 μg/mL gentamicin. At 6 hours post-infection, media was aspirated, and macrophages were lysed using TNT lysis buffer (20  mM Tris, 200  mM NaCl, 1% Triton [pH 8.0]). Lysate was then transferred to 96-well plates and assayed for luciferase activity by luminometry (Synergy HT; BioTek, Winooski, VT).

Acknowledgements

Research reported in this publication was supported by funding from the National Institutes of Health (T32GM007215 to HBS, R01AI137070 to J-DS, R01AI073843 to EPS, 1P01AI063302, and 1R01AI27655 to DAP, and K22AI144031 to SHL), the National Academies of Sciences, Engineering, and Medicine (Ford Foundation Fellowship to RR-L), the University of California Dissertation-Year Fellowship (to RR-L), and the Searle Scholars Program (to SHL). VMRR holds a Postdoctoral Enrichment Program Award from the Burroughs Wellcome Fund and acknowledges support from the Academic Pathways Postdoctoral Fellowship at Vanderbilt University and the Howard Hughes Medical Institute Hanna H Gray Fellows Program. Work at the Molecular Foundry was supported by the Office of Science, Office of Basic Energy Sciences, of the U.S. Department of Energy under Contract No. DE-AC02-05CH11231.

Funding Statement

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Contributor Information

Samuel H Light, Email: samlight@uchicago.edu.

Sophie Helaine, Harvard Medical School, United States.

Gisela Storz, National Institute of Child Health and Human Development, United States.

Funding Information

This paper was supported by the following grants:

  • National Institutes of Health T32GM007215 to Hans B Smith.

  • National Institutes of Health R01AI137070 to John Demian Sauer.

  • National Institutes of Health R01AI073843 to Eric P Skaar.

  • National Institutes of Health 1P01AI063302 to Daniel A Portnoy.

  • National Institutes of Health 1R01AI27655 to Daniel A Portnoy.

  • National Institutes of Health K22AI144031 to Samuel H Light.

  • National Academies of Sciences, Engineering, and Medicine Ford Foundation Fellowship to Rafael Rivera-Lugo.

  • University of California Dissertation-Year Fellowship to Rafael Rivera-Lugo.

  • Kinship Foundation Searle Scholars Program to Samuel H Light.

  • Howard Hughes Medical Institute Hanna H. Gray Fellows Program to Valeria M Reyes Ruiz.

  • Burroughs Wellcome Fund Postdoctoral Enrichment Program to Valeria M Reyes Ruiz.

  • Vanderbilt University Academic Pathways Postdoctoral Fellowship to Valeria M Reyes Ruiz.

  • Department of Energy DE-AC02-05CH11231 to Sara Tejedor-Sanz, Caroline M Ajo-Franklin.

Additional information

Competing interests

No competing interests declared.

No competing interests declared.

is a co-inventor on a filed patent describing the use of NOX. (US Patent App. 15/749,218).

Author contributions

Conceptualization, Investigation, Supervision, Writing – original draft.

Conceptualization, Investigation.

Investigation.

Conceptualization, Investigation, Writing – original draft.

Investigation.

Investigation.

Investigation.

Conceptualization, Investigation.

Investigation.

Investigation.

Investigation.

Conceptualization, Investigation, Writing – original draft.

Conceptualization, Funding acquisition, Investigation, Supervision, Writing – original draft.

Ethics

All animal work was performed in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. Protocols were reviewed and approved by the Animal Care and Use Committee at the University of California, Berkeley (AUP 2016-05-8811).

Additional files

Transparent reporting form

Data availability

All data generated or analyzed during this study are included in the manuscript and supporting files.

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Editor's evaluation

Sophie Helaine 1

In this study, authors report that a major role of respiration in Listeria monocytogenes pathogenicity, is to control redox balance (NAD+ regeneration) rather than generation of proton motive force. This is a new way of perceiving respiration that should be of interest to the microbiology community and broader readership.

Decision letter

Editor: Sophie Helaine1
Reviewed by: Andreas Bäumler2, Andrez Vazquez-torres3

Our editorial process produces two outputs: (i) public reviews designed to be posted alongside the preprint for the benefit of readers; (ii) feedback on the manuscript for the authors, including requests for revisions, shown below. We also include an acceptance summary that explains what the editors found interesting or important about the work.

Decision letter after peer review:

Thank you for submitting your article "Listeria monocytogenes requires cellular respiration for NAD+ regeneration and pathogenesis" for consideration by eLife. Your article has been reviewed by 3 peer reviewers, and the evaluation has been overseen by a Reviewing Editor and Gisela Storz as the Senior Editor. The following individuals involved in review of your submission have agreed to reveal their identity: Andreas Baumler (Reviewer #1); Andrez Vazquez-torres (Reviewer #3).

The reviewers have discussed their reviews with one another, and the Reviewing Editor has drafted this to help you prepare a revised submission.

Essential revisions:

(1) Maintaining redox balance was essential in tissue culture assays (Figure 5A and B), but only partially accounted for attenuation of a respiration-deficient mutant during growth in the murine liver and spleen. Seeing the relatively modest effect on the recovery of virulence associated with the heterologous expression of NOX in the liver, oxidative phosphorylation may still play an important role during growth in this tissue. Thus, the claim in the abstract and elsewhere in the paper "that NAD+ regeneration, rather than oxidative phosphorylation, represents the primary role of L. monocytogenes respiration" should be tempered down and authors should consider roles for respiration other than redox balance.

(2) The use of the heterologous NOX system can rescue a series of defects, from acetic acid production, plaque assay and macrophage growth, virulence in murine infection model, to menB complementation including lysis. This suggests dispensability of pmf-dependent processes in all the phenotypes listed above. Please test whether well-known pmf-dependent processes (transport, protein secretion and or motility) remain altered in respiration deficient mutants (menI, ∆QC, ∆QC fmn) expressing the NAD-regenerating NOX system.

3) The primary effect of fmn or QC mutations is to enhance the amount of oxidized (D)MK, which in turn might well impact the pool of NADH. However, one cannot rule out other effects due to imbalanced reduced/oxidized (D)MK per se. Since NADH dehydrogenases are the effectors of NADH oxidation, please test single or double ∆ndh1, ∆ndh2 and/or ndh mutants. Does heterologous expression of NOX rescue the phenotypes of such mutants?

(4) Add statistics for comparisons of wildtype and NOX-complemented ∆QC, ∆QC/fmnB, and ∆menB strains (Figures 4c, 4d, and 5c).

eLife. 2022 Apr 5;11:e75424. doi: 10.7554/eLife.75424.sa2

Author response

Essential revisions:

(1) Maintaining redox balance was essential in tissue culture assays (Figure 5A and B), but only partially accounted for attenuation of a respiration-deficient mutant during growth in the murine liver and spleen. Seeing the relatively modest effect on the recovery of virulence associated with the heterologous expression of NOX in the liver, oxidative phosphorylation may still play an important role during growth in this tissue. Thus, the claim in the abstract and elsewhere in the paper "that NAD+ regeneration, rather than oxidative phosphorylation, represents the primary role of L. monocytogenes respiration" should be tempered down and authors should consider roles for respiration other than redox balance.

Good point. We have re-worded the abstract and relevant part of the discussion to state that NAD+ regeneration is “a major role” of respiration.

(2) The use of the heterologous NOX system can rescue a series of defects, from acetic acid production, plaque assay and macrophage growth, virulence in murine infection model, to menB complementation including lysis. This suggests dispensability of pmf-dependent processes in all the phenotypes listed above. Please test whether well-known pmf-dependent processes (transport, protein secretion and or motility) remain altered in respiration deficient mutants (menI, ∆QC, ∆QC fmn) expressing the NAD-regenerating NOX system.

Thanks for the suggested control. We performed additional experiments which confirm that respiration-deficient mutants are less motile and that NOX expression does not impact this phenotype. These results are now presented in Figure 3—figure supplement 1.

3) The primary effect of fmn or QC mutations is to enhance the amount of oxidized (D)MK, which in turn might well impact the pool of NADH. However, one cannot rule out other effects due to imbalanced reduced/oxidized (D)MK per se. Since NADH dehydrogenases are the effectors of NADH oxidation, please test single or double ∆ndh1, ∆ndh2 and/or ndh mutants. Does heterologous expression of NOX rescue the phenotypes of such mutants?

Good point. The revised manuscript includes data in Figure 4A showing that the ∆ndh1/ndh2 mutant exhibits similar, NOX-rescuable, phenotypes in the plaque assay. The effect of NOX on this strain and the menB mutant (which lacks quinones) strongly suggests that NAD redox state and not is the primary driver of observed phenotypes.

4) Add statistics for comparisons of wildtype and NOX-complemented ∆QC, ∆QC/fmnB, and ∆menB strains (Figures 4c, 4d, and 5c).

Added.

Associated Data

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    Supplementary Materials

    Figure 1—source data 1. Source data for Figure 1B.
    elife-75424-fig1-data1.xlsx (10.9KB, xlsx)
    Figure 1—source data 2. Source data for Figure 1C.
    elife-75424-fig1-data2.xlsx (9.9KB, xlsx)
    Figure 1—figure supplement 1—source data 1. Source data for Figure 1—figure supplement 1A.
    elife-75424-fig1-figsupp1-data1.xlsx (10KB, xlsx)
    Figure 1—figure supplement 1—source data 2. Source data for Figure 1—figure supplement 1B.
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    Figure 2—source data 1. Source data for Figure 2A.
    elife-75424-fig2-data1.xlsx (11KB, xlsx)
    Figure 2—source data 2. Source data for Figure 2B.
    elife-75424-fig2-data2.xlsx (10KB, xlsx)
    Figure 2—source data 3. Source data for Figure 2C.
    elife-75424-fig2-data3.xlsx (9.6KB, xlsx)
    Figure 3—source data 1. Source data for Figure 3B.
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    Figure 3—source data 2. Source data for Figure 3C.
    elife-75424-fig3-data2.xlsx (9.8KB, xlsx)
    Figure 3—figure supplement 1—source data 1. Source data for Figure 3—figure supplement 1.
    elife-75424-fig3-figsupp1-data1.xlsx (9.4KB, xlsx)
    Figure 4—source data 1. Source data for Figure 4A.
    elife-75424-fig4-data1.xlsx (11.4KB, xlsx)
    Figure 4—source data 2. Source data for Figure 4B.
    elife-75424-fig4-data2.xlsx (10.1KB, xlsx)
    Figure 4—source data 3. Source data for Figure 4C.
    elife-75424-fig4-data3.xlsx (10.1KB, xlsx)
    Figure 5—source data 1. Source data for Figure 5B.
    elife-75424-fig5-data1.xlsx (11.2KB, xlsx)
    Figure 5—source data 2. Source data for Figure 5C.
    elife-75424-fig5-data2.xlsx (9.6KB, xlsx)
    Figure 5—source data 3. Source data for Figure 5D.
    elife-75424-fig5-data3.xlsx (9.3KB, xlsx)
    Transparent reporting form
    elife-75424-transrepform1.docx (111.2KB, docx)

    Data Availability Statement

    All data generated or analyzed during this study are included in the manuscript and supporting files.

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