Potassium response and homeostasis in Mycobacterium tuberculosis modulates environmental adaptation and is important for host colonization.

Successful host colonization by bacteria requires sensing and response to the local ionic milieu, and coordination of responses with the maintenance of ionic homeostasis in the face of changing conditions. We previously discovered that Mycobacterium tuberculosis (Mtb) responds synergistically to chloride (Cl-) and pH, as cues to the immune status of its host. This raised the intriguing concept of abundant ions as important environmental signals, and we have now uncovered potassium (K+) as an ion that can significantly impact colonization by Mtb. The bacterium has a unique transcriptional response to changes in environmental K+ levels, with both distinct and shared regulatory mechanisms controlling Mtb response to the ionic signals of K+, Cl-, and pH. We demonstrate that intraphagosomal K+ levels increase during macrophage phagosome maturation, and find using a novel fluorescent K+-responsive reporter Mtb strain that K+ is not limiting during macrophage infection. Disruption of Mtb K+ homeostasis by deletion of the Trk K+ uptake system results in dampening of the bacterial response to pH and Cl-, and attenuation in host colonization, both in primary murine bone marrow-derived macrophages and in vivo in a murine model of Mtb infection. Our study reveals how bacterial ionic homeostasis can impact environmental ionic responses, and highlights the important role that abundant ions can play during host colonization by Mtb.

Introduction

Ions are a fundamental component of organisms, playing roles in myriad biological processes. The ionic milieu surrounding a bacterium during infection varies with location and the immune response [1-7], and successful host colonization thus requires proper sensing and response to the local ionic milieu, and the ability to coordinate responses with the maintenance of ionic homeostasis in the face of changing conditions. For Mycobacterium tuberculosis (Mtb), pH ([H+] flux) is well-established as a critical signal during host colonization [8, 9], with the bacteria concurrently able to robustly maintain intrabacterial pH [10]. We have since identified chloride (Cl-) as an ionic cue important for Mtb [2], but it remains an open question what other abundant ions may flux during Mtb colonization, and how bacterial ionic homeostasis may affect response to environmental ionic cues. Mtb is a bacterium of immense public health importance, being the leading cause of death from infectious diseases worldwide [11]. Uncovering facets of the local environment that the bacteria respond to, and how fundamental aspects of Mtb biology relate to environmental response and colonization success, is critical for comprehension of Mtb-host interactions and has the potential to reveal novel nodes that can be targeted for therapeutic purposes.

Our previous discovery of Cl- as a novel environmental signal that Mtb responds to in synergy with pH indicated the significant role that flux and homeostasis of abundant ions can play during Mtb infection and disease [2]. In this context, potassium (K+), the most abundant intracellular cation in both mammalian and bacterial cells, stands out as a compelling candidate for study. In mammalian systems, K+ has fundamental roles in processes as diverse as renal function, muscle contraction, and neuronal information transmission [12-15]. There is also increasing appreciation for the importance of K+ in non-excitable cells, including in epithelial and immune cells in the lung [16, 17]. In contrast, studies on K+ in bacterial systems have predominantly focused on its role in osmoprotection [18]. However, results from a few studies have begun to hint at the broader importance of K+ in influencing bacterial pathogenicity and disease outcome. For example, higher environmental K+ concentrations ([K+]) increased expression of virulence factors and host cell invasion by the food-borne pathogen Salmonella enterica [19]. Inactivation of the Trk K+ uptake system in S. enterica further resulted in defects in effector protein secretion through the bacterium’s type III secretion system, and attenuation in virulence in both murine and chick models of infection [20]. A bacterial K+ uptake system has been shown to be essential for Helicobacter pylori gastric colonization [21], and K+ has also been shown to be part of a signal cascade that enables coordination of bacterial metabolic states in a Bacillus subtilis biofilm [22]. Mtb possesses two K+ uptake systems and one K+ efflux system [23-25], but the role of K+ in Mtb infection biology has been largely unstudied. How does Mtb respond transcriptionally to local changes in [K+], and how may this response be linked to the bacterial response to other environmental cues? What is the impact of perturbation of bacterial K+ homeostasis on successful host colonization by Mtb?

In this study, we show that Mtb has a unique transcriptional response to changes in environmental [K+]. While the pH and Cl- response regulator PhoPR does not affect Mtb response to external K+, the novel transcriptional repressor Rv0500A regulates bacterial response not just to pH and Cl-, but also K+. By using a K+-responsive fluorescent reporter Mtb strain in macrophage infections, we find that K+ in the phagosome is not limiting, and instead increases during phagosome maturation. Disruption of Mtb K+ homeostasis by deletion of the Trk K+ uptake system (ΔceoBC) results in dampening of the bacterial response to pH and Cl-, revealing the links between environmental ionic responses and bacterial ionic homeostasis. Finally, we show that the ΔceoBC mutant is attenuated for host colonization, both in primary murine bone marrow-derived macrophages and in vivo in a murine model of Mtb infection.

Results and discussion

Unique Mtb gene transcription signature in response to changes in environmental K+ levels

To elucidate the global transcriptional response of Mtb to changes in environmental [K+], we performed RNA sequencing (RNAseq) on Mtb exposed for 4 hours to K+-free 7H9 media, and compared it to samples in standard 7H9 media ([K+] = 7.35 mM). We found that 43 genes were upregulated and 66 genes downregulated (>2-fold, p<0.05) in response to low [K+] (S1 and S2 Tables). The upregulated gene list represented a unique gene set, with slight overlap with genes upregulated in response to high [Cl-], but otherwise little overlap when compared to other known environmental regulons (Table 1) [2, 8, 26–28]. Among the strongest upregulated genes were those belonging to the kdpFABC operon. These genes encode the inducible K+ uptake ATPase KpdFABC, and their robust upregulation served to affirm their function in low environmental [K+] [24]. Interestingly, several genes related to iron uptake were repressed upon Mtb exposure to low environmental [K+] (S2 Table). These included five mycobactin genes (mbtB, mbtC, mbtD, mbtI, and mbtK), as well as the iron-regulated transporter genes irtA and irtB. Comparison to the previously reported gene set downregulated under conditions of high iron revealed a significant overlap (Table 1) [27]. Oxidative stress is known to induce the expression of iron uptake genes, including the mbt genes [26], and we accordingly also observed an overlap between the low [K+] downregulated gene set and genes upregulated upon exposure to oxidative stress (Table 1). Quantitative real time PCR (qRT-PCR) of candidate genes confirmed the RNAseq data (Fig 1). In addition, no expression differences in the candidate genes were observed in sodium (Na+)-free media, reinforcing the specificity of the K+ response regulon (S1 Fig).

Table 1

Comparison of low [K+] response regulon to different environmental response regulons.

In vitro stimulus	Genes in reference lista	Overlap with upregulated gene list in K+-free 7H9	Overlap with downregulated gene list in K+-free 7H9
Acid stressc	291	2	4
Oxidative stressd	142	0	21b
High irone	66	1	19b
Hypoxiaf	50	3	0
High [Cl-]g	32	5b	1

a All reference lists refer to upregulated gene sets, except for the high iron set, which refers to the downregulated gene set.

b Overlap for these comparisons are significant at p<0.01 (hypergeometric distribution).

c Data from Rohde et al. [8]

d Data from Voskuil et al. [26]

e Data from Rodriguez et al. [27]

f Data from Park et al. [28]

g Data from Tan et al. [2]

Fig 1

Transcriptional response of Mtb to low environmental [K+].

(A and B) qRT-PCR of gene expression in WT grown in K+-free 7H9, pH 7, compared to standard 7H9, pH 7, for 4 hours. Upregulated genes are shown in (A), and downregulated genes are shown in (B). Data are shown as means ± SD from 3 technical replicates, representative of 2–3 independent experiments.

These transcriptional data reveal a significant response of Mtb to limiting external [K+], with a unique signature of upregulated genes. The unexpected overlap with the iron and oxidative stress response regulons in the downregulated gene set provides an intriguing base for future studies.

kdpF’::GFP functions as a specific reporter of Mtb response to environmental K+ levels

The transcriptional data above demonstrated the very robust induction of the kdpFABC operon upon exposure to low environmental [K+] [24]. To aid further study of Mtb response to K+, we thus generated a fluorescent K+-responsive Mtb strain by cloning the promoter region of kdpF immediately upstream of GFP in a replicating plasmid, and transforming this kdpF’::GFP construct into Mtb. As expected, reporter GFP fluorescence was induced upon growth in low [K+], with signal intensity increasing with decreasing [K+] (Fig 2A). Testing of the kdpF’::GFP reporter in several other conditions known to be environmental cues for Mtb (acidic pH, high [Cl-], high osmolarity, and hypoxia) revealed no fluorescence induction, illustrating its specificity (Fig 2B and 2C). The lack of response to osmolarity is intriguing, as the KdpFABC system is canonically upregulated during exposure to high environmental osmolarity, in addition to limiting [K+] [29-31]. There is however precedence for a Kdp system being non-responsive to osmolarity, with this phenotype demonstrated for Kdp homologs in the cyanobacterium Anabaena and the extremophile Deinococcus radiodurans [32, 33]. In agreement with our results, previous studies examining the response of Mtb to osmolytes (NaCl, KCl, and sucrose) had not observed changes in kdpFABC gene expression [2, 34]. Mtb is extremely robust at coping with osmolarity, and it is possible that it utilizes distinct systems for osmolarity response. Indeed an osmosensory pathway regulated by the eukaryotic-like serine/threonine protein kinase PknD has been described for Mtb [34].

Fig 2

kdpF’::GFP functions as a specific reporter of Mtb response to environmental K+ levels.

(A) Mtb response to K+ is concentration-dependent. CDC1551(kdpF’::GFP, smyc’::mCherry) was grown in standard 7H9 broth, pH 7.0, or in K+-free 7H9 broth, pH 7.0, supplemented with indicated amounts of K+. Samples were taken at indicated time points, fixed, and GFP induction analyzed by FACS. Data are shown as means ± SD from 3 independent experiments. (B-C) kdpF’::GFP induction is specific. CDC1551(kdpF’::GFP, smyc’::mCherry) was grown in 7H9 broth, pH 7.0, supplemented with 250 mM NaCl (green triangles) or 300 mM sucrose (blue inverted triangles), in 7H9 broth, pH 5.7 (red squares), or in K+-free 7H9 broth, pH 7.0 (dotted black line, circles) (B). In (C), CDC1551(kdpF’::GFP, smyc’::mCherry) was grown in media in stirred, aerated, cultures, before exposure to 0.5% O2 for 6 days. The hypoxia responsive strain, CDC1551(hspX’::GFP, smyc’::mCherry), was used as a control. All samples were analyzed as in (A), and data are shown as means ± SD from 3 independent experiments. (D) KdpDE inactivation abolishes kdpF’::GFP induction in low [K+]. WT, ΔkdpDE, or kdpDE* (complemented mutant) Mtb expressing the kdpF’::GFP reporter were grown in standard 7H9 broth, pH 7.0, or in K+-free 7H9 broth, pH 7.0, supplemented with 0.05 mM KCl. All samples were analyzed as in (A), and data are shown as means ± SD from 3 independent experiments.

Expression of kdpFABC is expected to be modulated by the two-component system KdpDE, based on homology to model systems such as Escherichia coli [35], and from Mtb studies examining regulatory partners of KdpD and the effect of over-expression of kdpE [24, 36]. As expected by this regulation, induction of kdpF’::GFP signal in the presence of low environmental [K+] was lost in a ΔkdpDE Mtb mutant, with genetic complementation successfully restoring the WT phenotype (Fig 2D). These data demonstrate the robustness of the kdpF’::GFP reporter as a specific and sensitive K+ reporter for Mtb, and support its utility for analyses of Mtb K+ response.

Distinct and novel shared regulatory mechanisms influence Mtb response to abundant ions

With the kdpF’::GFP K+ reporter in hand, we next sought to determine if regulation of Mtb response to K+ is linked to the bacterial response to other abundant environmental ions, in particular H+ (acidic pH) and Cl-. Acidic pH is well-established as a critical environmental signal for Mtb during host colonization [8, 10, 37], and we had discovered that the bacteria also respond transcriptionally to external Cl-, with significant overlap in the pH and Cl- response regulons [2]. Mtb response to pH and Cl- is synergistic [2], and regulation of Mtb response to pH and Cl- is closely linked, with both shared activators and repressors. In particular, we had previously found that the two-component regulator PhoPR is a key activator of Mtb response to both acidic pH and Cl-, with attenuation of response upon PhoPR inactivation [2]. Conversely, in an initial screen for other genes controlling Mtb response to Cl- that utilized transposon libraries generated in the background of our previously described Cl- and pH-sensitive rv2390c’::GFP reporter Mtb strain [2], we identified Rv0500A as a novel repressor of Mtb response to acidic pH and Cl-. Specifically, inactivation of Rv0500A was found to enhance expression of the rv2390c’::GFP reporter upon exposure to the inducing signals of Cl- and/or acidic pH (Fig 3A).

Fig 3

Distinct and novel shared regulatory mechanisms influence Mtb response to abundant ions.

(A) rv0500A disruption enhances Mtb response to acidic pH and high [Cl-]. WT, rv0500A::Tn, or rv0500A* (complemented mutant) Mtb carrying the Cl-/pH responsive rv2390c’::GFP reporter were grown in pH 7 or pH 5.7 media, ± 250 mM NaCl, for 9 days. GFP signal in fixed samples was measured by FACS, with fold signal induction compared to the corresponding strain grown in pH 7 control media. Data are shown as means ± SD from 3–4 independent experiments. p-values were obtained with an unpaired t-test, * p<0.05, ** p<0.01, *** p<0.001. (B) PhoP does not affect Mtb response to K+. WT or phoP::Tn Mtb carrying the K+-responsive kdpF’::GFP reporter were grown in standard 7H9 media (control) or K+-free 7H9. Samples were taken at indicated time points, fixed, and GFP induction analyzed by FACS. Data are shown as means ± SD from 3 independent experiments. (C) rv0500A disruption enhances Mtb response to low [K+]. WT, rv0500A::Tn, or rv0500A* Mtb carrying the kdpF’::GFP reporter were grown in standard 7H9 media or K+-free 7H9 for 9 days. GFP reporter induction was determined as in (A). Data are shown as means ± SD from 3–5 independent experiments. p-values were obtained with an unpaired t-test, ** p<0.01, *** p<0.001.

Expression of the K+-sensitive kdpF’::GFP reporter in a phoP transposon mutant (phoP::Tn) revealed no difference in signal induction upon exposure of the bacteria to low [K+] as compared to WT Mtb, indicating that the PhoPR regulator does not contribute to regulation of Mtb K+ response (Fig 3B). In contrast, kdpF’::GFP expression was enhanced in a rv0500A transposon mutant (rv0500A::Tn) when the bacteria were grown in K+-free media (Fig 3C), similar to the enhancement of rv2390c’::GFP reporter signal observed during exposure of the rv0500A::Tn mutant to high [Cl-] and/or acidic pH media (Fig 3A). We note that the rv2390c’::GFP reporter does not respond to low external [K+] (S2 Fig), in accord with its previously described high specificity for Cl- and pH [2].

To further explore the role of Rv0500A in Mtb response to ionic signals, we expressed and purified recombinant Rv0500A (S3 Fig), and tested for its ability to directly bind the rv2390c and kdpF promoters. As shown in Fig 4A, a clear shift was observed in electrophoretic mobility shift assays (EMSAs) conducted with Rv0500A and the rv2390c promoter, demonstrating binding of the protein to the DNA fragment. In contrast, we did not observe a shift when the kdpF promoter was used (Fig 4B). EMSAs with separated 5’ and 3’ sections of the rv2390c promoter showed a distinct shift with the 3’ but not the 5’ section, further illustrating the specificity of Rv0500A binding (Fig 4C). Together, these data demonstrate that Rv0500A binds directly to specific DNA regions, and indicate that Rv0500A regulation of kdpF may be indirect, as opposed to its direct effect on rv2390c expression.

Fig 4

Rv0500A binds directly to the rv2390c promoter.

(A and B) Rv0500A binds directly to the rv2390c promoter but not the kdpF promoter. Electrophoretic mobility shift assays (EMSAs) were performed using purified recombinant N-terminally 6x-His-tagged Rv0500A and DNA probes for the rv2390c promoter (A) or the kdpF promoter (B). The highest concentration binding reaction contained 0.1 μM His-Rv0500A followed by two-fold serial dilutions. A control with no His-Rv0500A protein added is shown in the first lane. All DNA probes were labeled with IRDye 700. Data are representative of 2–3 independent experiments. (C) Rv0500A binds directly to a 3’ section of the rv2390c promoter. The schematic at the top shows the “split” promoter regions. EMSAs were performed as above with the 5’ (left panel) or 3’ (right panel) sections of the rv2390c promoter. Data are representative of 2 independent experiments.

Our findings demonstrate that Mtb response to the different ionic signals of K+, Cl-, and pH are controlled by both distinct and shared regulatory mechanisms, and illustrate the complexity of Mtb integration of its response to disparate environmental cues. These data further reveal Rv0500A as a novel transcription regulator that represses Mtb response to these abundant ionic signals, and additional studies focused on analysis of Rv0500A function are currently in progress.

Expression of kdpF’::GFP is downregulated during macrophage infection

pH and Cl- are key signals present in the Mtb phagosome [2, 8, 37], and a previous study had indicated that [K+] in the lysosome decreases as a counterbalance to the influx of H+ [38]. While K+ levels in Mtb-containing phagosomes had been queried in an earlier intriguing study utilizing x-ray fluorescence microscopy, conclusions regarding changes in [K+] could not be drawn from the values obtained, and the resolution of the method had precluded differentiation of levels in the bacterium itself versus in the phagosomal compartment [39]. In the context of neutrophil phagosomes, there has been much debate as to whether [K+] increase is important upon generation of the oxidative burst [40-43]. Given our findings of both distinct and shared regulatory mechanisms underlying Mtb response to acidic pH, Cl-, and K+, we next utilized our kdpF’::GFP reporter Mtb strain as a unique tool for interrogating the relative environmental [K+] the bacteria are exposed to during macrophage infection.

For this assay, we used our previously established dual fluorescent reporter strategy, in which a constitutively expressed smyc’::mCherry is placed downstream of the environmental-responsive reporter (here kdpF’::GFP), enabling visualization of all bacteria during infection [2, 37, 44]. Infection of primary murine bone marrow-derived macrophages with this dual kdpF’::GFP, smyc’::mCherry reporter Mtb strain revealed a decrease in kdpF’::GFP reporter signal over the course of eight days in both resting and activated macrophages (Fig 5A and 5B). This downregulation in kdpF’::GFP signal was further emphasized when the reporter Mtb were grown in low environmental [K+] prior to infection (Fig 5C and 5D).

Fig 5

kdpF’::GFP is downregulated during macrophage infection.

(A and B) Expression of kdpF’::GFP is downregulated during Mtb infection of macrophages. Resting or activated macrophages were infected with CDC1551(kdpF’::GFP, smyc’::mCherry). (A) shows 3D confocal images of the beginning (2 hrs) and end (8 days) of infection. All bacteria are marked in red (smyc’::mCherry), the reporter is shown in green (kdpF’::GFP), and nuclei are shown in grayscale (DAPI). Scale bar 5 μm. (B) shows quantification of the GFP/μm3 signal for each bacterium measured from multiple 3D confocal images. Each point on the graph represents a bacterium or a tight cluster of bacteria (circles—Mtb in resting macrophages, squares—Mtb in activated macrophages). p-values were obtained with a Mann-Whitney statistical test, and is in comparison to the corresponding 2 hr data set in each case. *** p<0.001, **** p<0.0001. (C and D) Pre-growth of Mtb in K+-free media enhances kdpF’::GFP reporter signal decrease during infection. CDC1551(kdpF’::GFP, smyc’::mCherry) was grown in K+-free media for 6 days prior to infecting resting or activated murine macrophages. (C) shows 3D confocal images of the infection at the beginning (2 hrs) and end (8 days) of the infection. All bacteria are marked in red (smyc’::mCherry), the reporter is shown in green (kdpF’::GFP), and nuclei are shown in grayscale (DAPI). Scale bar 5 μm. (D) shows quantification of the bacterial GFP/μm3 signal, determined as in (B).

These data strongly indicate that K+ is not limiting within the Mtb phagosome, similar to conclusions reached for the Salmonella-containing vacuole that were based on transcriptional studies showing no upregulation of bacterial K+ transport systems in intracellular Salmonella [45]. Our findings further suggest that the outward K+ flux countering acidification of lysosomes previously observed does not function in the context of the Mtb phagosome [38], in accord with Mtb prevention of complete acidification of its phagosome [46, 47].

Intraphagosomal K+ concentration increases during phagosomal maturation

To further examine [K+] changes in the maturing phagosome with an independent approach, we utilized the K+-sensitive compound Asante K+ Green 4 (APG4) [22, 48], which we covalently linked to 3 μm silica beads, together with Alexa Fluor 594 (AF594) as a calibration fluorophore [2]. These K+ sensor beads fluoresced specifically as [K+] increased, with no APG4 fluorescence induced by changes in sodium concentration or pH (Fig 6A and 6B). In agreement with the kdpF’::GFP reporter assay above, tracking of APG4/AF594 bead fluorescence upon addition to primary murine bone marrow-derived macrophages showed that K+ was not limiting in the maturing macrophage phagosome; instead, phagosomal [K+] increased as the compartment matured in both resting and activated macrophages (Fig 6C). Inhibition of H+-ATPase activity with concanamycin A inhibits phagosome acidification and had previously been shown to affect phagosome maturation [49]. We found that concanamycin A treatment resulted in very significant loss of the increase observed in APG4/AF594 signal in mock-treated samples, further supporting the conclusion that [K+] increases during phagosome maturation (S4 Fig).

Fig 6

Intraphagosomal K+ concentration increases during phagosomal maturation.

(A and B) APG4/AF594 beads respond specifically to [K+]. APG4/AF594 beads were placed in buffer containing specific [K+] or [Na+] (A), or in buffer with 100 mM Bis-Tris adjusted to the indicated pH with HCl (B). APG4 and AF594 fluorescence were measured on a microplate reader, and data are shown as means ± SD from 4 wells, representative of 2–3 independent experiments. (C and D) Intraphagosomal [K+] increases during phagosomal maturation independent of an oxidative burst. APG4/AF594 beads were added to resting or activated murine bone marrow-derived macrophages (MØ) from WT (C and D) or gp91phox-/- mice (D), and fluorescence tracked with a microplate reader over time. Sensor beads were also added to wells containing only media, with no macrophages (“beads only, no MØs”). Data are shown as means ± SD from 4 wells, representative of 3–5 independent experiments.

As the oxidative burst has been implicated as a driving factor in [K+] increase within neutrophil phagosomes [40], we next asked if macrophages deficient in NADPH oxidase function (gp91phox-/-) would exhibit the increase in phagosomal [K+] observed in WT macrophages. We found that gp91phox-/- macrophages retained their ability to increase phagosomal [K+], indicating that the oxidative burst is not required for this phenotype in macrophages (Fig 6D). These findings add to the knowledge base of changes in the ionic milieu during macrophage phagosome maturation, and further studies are required to delineate the channels/transporters that mediate this K+ flux.

Mtb K+ homeostasis augments the bacterial response to Cl- and pH

Having established that [K+] increases during macrophage phagosome maturation, similar to increases in [Cl-] and [H+] [2], and in light of the interplay in Mtb response to these ions illustrated by our results above with Rv0500A, we next sought to determine if disruption of Mtb K+ homeostasis would affect bacterial response to Cl- and pH. Mtb has two K+ uptake systems: (i) Kdp, a high affinity, inducible system, and (ii) Trk, a constitutive, low-moderate affinity system [23, 50, 51]. Given our finding that K+ is not limiting within the Mtb phagosome, we focused our studies here on the Trk K+ uptake system, encoded by the ceoB and ceoC genes.

A ΔceoBC Mtb mutant was constructed via homologous recombination, and the Cl- and pH-responsive rv2390c’::GFP reporter introduced into the strain [2]. In agreement with the role of CeoBC as a constitutive, low-moderate affinity K+ uptake system, tests with the kdpF’::GFP reporter indicated that the ΔceoBC mutant is slightly more sensitive to low environmental [K+] (S5 Fig). The ΔceoBC mutant had no growth defect in standard broth, or in high [Cl-], acidic pH, or low [K+] media, as compared to WT Mtb (Fig 7A). Strikingly however, the ΔceoBC mutant demonstrated significantly decreased reporter GFP signal when grown in defined broth conditions with high [Cl-] and/or acidic pH, which was restored to WT levels upon genetic complementation (ceoBC*) (Fig 7B). To establish that an attenuated response to environmental [Cl-] and pH by the ΔceoBC mutant was a broader phenotype not restricted to rv2390c response, we performed qRT-PCR on several other Cl- response regulon genes [2]. As shown in Fig 7C, the transcriptional response of the ΔceoBC mutant was dampened in each case, although the magnitude of reduction varied from gene to gene.

Fig 7

Mtb K+ homeostasis augments the bacterial response to Cl- and pH.

(A) Mtb ΔceoBC mutant growth during environmental stress. WT or ΔceoBC mutant Mtb were grown in standard pH 7.0 media ± 250 mM NaCl, pH 5.7 media, or in K+-free 7H9 media, pH 7.0, supplemented with 0.1 mM KCl, and growth tracked over time. Data are shown as mean ± SD from 3 independent experiments. (B and C) Mtb ΔceoBC mutant has an attenuated response to Cl- and acidic pH. In (B), WT, ΔceoBC, or ceoBC* (complemented mutant) Mtb expressing the rv2390c’::GFP reporter were grown in pH 7 or pH 5.7 media, ± 250 mM NaCl. GFP signal in fixed samples was measured by FACS, with fold signal induction compared to the corresponding strain grown in pH 7 control media. Data are shown as means ± SD from 3 independent experiments. p-values were obtained with an unpaired t-test, ** p<0.01, *** p<0.001, **** p<0.0001. (C) shows qRT-PCR of gene expression changes in WT, ΔceoBC, or ceoBC* 4 hrs post-exposure to pH 7 media ± 250 mM NaCl. Fold induction is as compared to gene expression in pH 7 media for each strain. Data are shown as mean ± SD from 3 technical replicates, representative of 2 independent experiments. p-values were obtained with an unpaired t-test, * p<0.05, *** p<0.001, **** p<0.0001. (D) Maintenance of intrabacterial pH in the ΔceoBC mutant. WT or ΔceoBC mutant Mtb were incubated for 1 hour with 5-chloromethylfluorescein diacetate, before washing and exposure to PBS or K+-free PBS containing 0.05% tween 80, at pH 7.3 or pH 5.7. Fluorescence was read with a microplate reader at Ex. 450 nm and 490 nm, and Em. at 520 nm. 10 μM of the ionophore nigericin was added to assay control samples. Data were normalized as a percentage of the fluorescence ratios (Ex. 490 nm/Ex, 450 nm) observed in PBS, pH 7.3, for a given strain, and shown as means ± SD from 3 wells. The results are representative of 4 independent experiments. (E) ΔceoBC mutant maintains membrane potential during environmental stress. WT or ΔceoBC mutant Mtb were resuspended in pH 7 or pH 5.7 media, or in K+-free 7H9, pH 7 media containing 0.5 mg/l of rhodamine 123. 50 μM of the protonophore carbonyl cyanide m-chlorophenylhydrazone was added to assay control samples. Fluorescence decay was tracked every 10 minutes for 4 hours with a microplate reader at Ex. 485 nm/Em. 527 nm, and normalized to initial probe fluorescence for each strain and condition. The assay was repeated 4 times, and data are shown as means ± SD from 8 wells across 2 independent experiments.

To test that the phenotypes observed were due more directly to disruption of bacterial K+ homeostasis versus possible downstream effects on the bacterial membrane from deletion of an ion transport system, we first assessed the ability of the ΔceoBC mutant to maintain intracellular pH during growth in acidic conditions. As previously described, the pH-sensitive, cell-permeable, dye 5-chloromethylfluorescein diacetate (CMFDA) is rendered cell-impermeant once in the cytoplasm of cells, and thus enables measurement of intracellular pH in a ratiometric manner, as fluorescein is pH sensitive when excited at 490 nm, but pH insensitive when excited at 450 nm (emission at 520 nm in both cases) [52]. We found that the ΔceoBC mutant maintained intracellular pH as well as WT Mtb, even when exposed to a pH 5.7 environment (Fig 7D). Treatment of the bacteria with nigericin, an ionophore, resulted in the expected decrease in excitation 490 nm/450 nm (emission 520 nm) fluorescence ratio in the presence of external acidity, and served as an assay control (Fig 7D).

Next, we tested for defects in maintenance of membrane potential. The cationic dye Rhodamine 123 allows relative determination of cellular membrane potential, with increased uptake, and consequently greater fluorescence decay over time, in cells with higher membrane potential [53, 54]. In standard pH 7 growth media, WT and ΔceoBC Mtb had similar membrane potential (Fig 7E). Exposure of Mtb to an acidic external pH resulted in the expected membrane depolarization, but here again no difference in membrane potential was observed between WT and ΔceoBC Mtb (Fig 7E). Membrane potential of the ΔceoBC mutant was also not different to that of WT Mtb in conditions of low environmental [K+] (Fig 7E). The effect of protonophore (carbonyl cyanide m-chlorophenylhydrazone, CCCP) addition was analyzed as a control, and resulted in the expected membrane depolarization and decrease in relative fluorescence decay in each condition (Fig 7E).

These results reveal the novel concept that bacterial K+ homeostasis can impact on Mtb response to ionic signals in its local environment, independent of broader effects on maintenance of membrane potential. This new concept highlights the complexity of bacterial K+ biology, and the intimate relationship between ionic homeostasis and ionic signal response. It further raises the intriguing suggestion that targeting of Mtb K+ homeostasis will have far-reaching adverse consequences for the bacterium that extend beyond K+ balance alone.

Disruption of K+ homeostasis attenuates Mtb colonization ability in macrophages and in vivo

The changing [K+] in the phagosome and the observed impairment in bacterial response to pH and Cl- in the ΔceoBC mutant suggests that this mutant may be attenuated in colonization of macrophages. To test this, we infected primary murine bone marrow-derived macrophages with WT, ΔceoBC, or ceoBC* Mtb, and tracked bacterial growth over time. We found that the ΔceoBC mutant was significantly attenuated in its ability to colonize macrophages, with the bacterial load recovered 6 days post-infection only about half that obtained from WT or ceoBC*-infected samples (Fig 8A). In agreement with our results, we note that ceoB mutants had previously been found to be under-represented in a transposon site hybridization-based screen for Mtb genes important for survival/growth in macrophages [55]. Utilization of the rv2390c’::GFP, smyc’::mCherry reporter in the various strains further showed that rv2390c’::GFP signal was decreased in the ΔceoBC mutant as compared to that in WT or ceoBC* Mtb during infection of activated macrophages (Fig 8B and 8C). These reporter data suggest that the impaired response of the ΔceoBC mutant to Cl- and pH observed in broth is similarly exhibited during macrophage infection.

Fig 8

Disruption of bacterial K+ homeostasis decreases Mtb colonization of macrophages.

(A) Mtb ΔceoBC mutant is attenuated for macrophage colonization. Murine bone marrow-derived macrophages were infected with WT, ΔceoBC, or ceoBC* (complemented mutant) Mtb, and CFUs tracked over time. Data are shown as means ± SD from 5–6 wells, representative of 3–4 independent experiments. (B and C) Mtb ΔceoBC mutant exhibits decreased rv2390c’::GFP induction response during macrophage infection. Activated murine bone marrow-derived macrophages were infected with WT, ΔceoBC, or ceoBC* Mtb expressing the rv2390c’::GFP, smyc’::mCherry reporter. (B) shows 3D confocal images of the beginning (2 hrs) and end (8 days) of infection. All bacteria are marked in red (smyc’::mCherry), the reporter is shown in green (rv2390c’::GFP), and nuclei are shown in grayscale (DAPI). Scale bar 5 μm. (C) shows quantification of the GFP/μm3 signal for each bacterium measured from multiple 3D confocal images. Each point on the graph represents a bacterium or a tight cluster of bacteria (black circles—WT, red squares– ΔceoBC, blue triangles—ceoBC*). p-values were obtained with a Mann-Whitney statistical test. N.S. not significant, **** p<0.0001.

Finally, to examine the effect of disrupting Mtb K+ homeostasis on the bacterium’s ability to colonize a whole animal host, we infected C57BL/6J WT mice with WT, ΔceoBC, or ceoBC* Mtb, and analyzed bacterial load and histopathology two and four weeks post-infection. The ΔceoBC mutant was significantly attenuated for host colonization at both time points, with bacterial loads 3–4 fold less than that obtained from infections with WT or ceoBC* (Fig 9A). Histopathology in ΔceoBC-infected animals was correspondingly less severe, with decreased cellular infiltration and better maintenance of clear alveolar air spaces (Fig 9B). These results demonstrate a role for the CeoBC K+ uptake system in Mtb pathogenesis, and underscore the importance of K+ homeostasis for the bacterium in successfully establishing host colonization.

Fig 9

Disruption of bacterial K+ homeostasis results in attenuation of Mtb growth in vivo.

(A) Mtb ΔceoBC mutant is attenuated for colonization in a murine infection model. C57BL/6J WT mice were infected with WT, ΔceoBC, or ceoBC* (complemented mutant) Mtb, and lung homogenates plated for CFUs 14 or 28 days post-infection. p-values were obtained with a Mann-Whitney statistical test. * p<0.05, ** p<0.01. (B) Lung pathology in infected mice. Lungs obtained from infected animals 14 or 28 days post-infection were fixed and processed for hematoxylin and eosin staining. Scale bar 200 μm.

Concluding remarks

From the macrophage phagosome to the granuloma, Mtb is exposed to a complex environmental milieu that plays a significant role in its infection biology. Signals present reflect cellular and tissue location, as well as the host immune status [1-4], and Mtb must coordinate its response to disparate signals to ensure adaptation and continued survival and growth. Our discovery that disruption of the CeoBC K+ uptake system results in attenuation of Mtb response to external pH and Cl- levels, independent of changes in membrane potential, reveals the close links between ionic homeostasis and bacterial response to diverse environmental cues. Together with our previous findings demonstrating the synergistic response of Mtb to acidic pH and Cl- [2], these results highlight the need to examine Mtb ionic homeostasis and response beyond the study of individual signals in isolation. Our discovery of Rv0500A as a shared repressor affecting Mtb response to pH, Cl-, and K+ begins to shed mechanistic insight into this key facet, and studies to elucidate the role of Rv0500A during infection are ongoing. Interestingly, a global transcription factor study by Rustad et al. identified over-expression of glnR (rv0818), a master nitrogen metabolism regulator [56, 57], as inducing transcription of kdpFABC in standard broth conditions where this K+ uptake system is not normally upregulated [36]. It will thus also be intriguing in future studies to assess the connections that may exist between K+ signals and nitrogen metabolism proposed by this data. In addition, the observed attenuation of the ΔceoBC mutant in host colonization suggests that uncovering how Mtb integrates ionic homeostasis and response to environmental cues represents an important area for understanding mechanisms that enable effective bacterial colonization of the host, essential for complete comprehension of Mtb pathogenesis. Our findings are likely also applicable to other bacterial pathogens, given the widespread presence of the Trk (CeoBC) K+ uptake system, which in the case of Salmonella has also been shown to play an important role during infection [20].

More broadly, studies on the role of ions in host-pathogen interactions have most often focused on scarce ions that can be sequestered by the host, such as iron, zinc, and manganese [6, 7, 58, 59]. These ions are clear targets in understanding bacterial pathogenesis, given both their scarcity and their importance for bacterial and host physiology. Much less studied however has been the role that abundant ions, like K+ and Cl-, can play in infectious disease. While such ions are not a resource that bacteria have to “fight” their host for, we propose that their very abundance, inability to be sequestered by the host, varying levels in different cellular compartments and upon immune activation, and critical roles in host biology, make them ideal targets for exploitation by pathogens. Our findings of the change in [K+] during macrophage phagosome maturation, and of the specific transcriptional response of Mtb to K+, builds on our previous results with Cl- [2], and raise questions about how bacteria may exploit [K+] flux during infection. S. enterica presents a noteworthy example, given the reported increase in virulence factor expression upon exposure to higher environmental [K+] [19]. Might external K+ levels also affect the ability of Mtb to adapt to its local environment? It further remains to be elucidated when Mtb may experience limiting environmental [K+], and the possible link to iron and oxidative stress suggested by our transcriptional data is an intriguing finding that merits further study. Of note, K+ levels have been implicated in macrophage immune responses, with inhibition of K+ channels reducing nitric oxide induction [60], and low intracellular K+ activating the NALP3 inflammasome [61]. K+ may thus function as a signal both for the host and the bacterium, and further studies are needed to determine crosstalk and balance in these processes during host-pathogen interactions.

We propose that further studies pursuing the novel concepts highlighted by our results here will provide important insight into how fundamental aspects of both Mtb and host biology are linked during the infection process, and reveal unique nodes that can be perturbed to shift the balance of infection.

Materials and methods

Ethics statement

All animal procedures followed the National Institutes of Health “Guide for the Care and Use of Laboratory Animals” standards. The Institutional Animal Care and Use Committee at Tufts University reviewed and approved all animal protocols (#B2016-37), in accordance with guidelines established by the Association for Assessment and Accreditation of Laboratory Animal Care, the US Department of Agriculture, and the US Public Health Service.

Mtb strains and culture

Mtb cultures were propagated as previously described [37]. Strains for in vitro assays were in the CDC1551 background, while strains for CFU enumeration in macrophages and in vivo were in the Erdman background. Mtb mutants and their complements were constructed as previously described [2]. The ΔceoBC mutation consisted of a deletion beginning 102 bp from the ceoB start codon through 73 bp from the ceoC stop codon, while the entire open reading frame was deleted for ΔkdpDE. The phoP::Tn mutant from BEI Resources (NR-14776) has been previously described [2, 37]. The rv0500A::Tn mutant was isolated from a Tn library generated in the background of a CDC1551(rv2390c’::GFP) strain via use of a mariner-based ϕMycoMarT7 phage [62, 63], with the Tn insertion 125 bp into the open reading frame.

RNA sequencing and qRT-PCR analyses

Log-phase (OD600 ~ 0.6) Mtb was used to inoculate standing, vented, T-25 flasks containing either 10 ml of standard 7H9, pH 7 medium ([K+] = 7.35 mM) or K+-free 7H9, pH 7 medium at OD600 = 0.3. K+-free 7H9 was made by replacing monopotassium phosphate with monosodium phosphate. To make Na+-free 7H9, disodium phosphate was replaced with dipotassium phosphate, monosodium glutamate with monopotassium glutamate, and sodium citrate with potassium citrate. The media was supplemented with 0.5% bovine serum albumin, 0.2% dextrose, and 14.5 mM KCl, and brought to pH 7 with KOH. Samples were collected 4 hours post-exposure and RNA isolation carried out as previously described [8]. Two biological replicates per condition were used for RNA sequencing. Library preparation using Ribo-Zero rRNA removal (bacterial) and TruSeq Stranded kits (Illumina) were performed by the Tufts University Genomics Core Facility. Barcoded samples were pooled and run on a single lane on an Illumina HiSeq 2500 (High Output v4) with single-end 100 bp reads. Data were analyzed using the SPARTA program [64]. qRT-PCR experiments were performed as previously described, except cDNA was synthesized from 250 ng of RNA without prior amplification [2, 37].

Fluorescent reporter Mtb strains and in vitro assays

The Cl- and pH-sensitive rv2390c’::GFP reporter has been previously described [2]. A similar approach was used to construct the K+-sensitive reporter kdpF’::GFP, with the 754 bp region immediately upstream of kdpF amplified by PCR and fused to GFPmut2 [2, 37]. The resulting kdpF’::GFP construct was then introduced into a vector containing the constitutively expressed smyc’::mCherry, and transformed into Mtb. Selection was carried out on 7H10 agar containing 25 μg/ml kanamycin, 50 μg/ml apramycin, or 50 μg/ml hygromycin B as appropriate.

Broth culture assays were conducted by growing Mtb in standing vented T-25 flasks in 10 ml of 7H9 buffered media as previously described [2], with addition of 250 mM NaCl or 300 mM sucrose as needed. To vary [K+], a specified amount of KCl was added to the K+-free 7H9. Antibiotics were added as necessary to maintain selection. The hypoxia assays were performed as previously described [2]. Mtb was fixed in 4% paraformaldehyde (PFA) in phosphate buffered saline (PBS) prior to fluorescence analysis. GFP was read on a BD FACSCalibur with subsequent data analysis using FloJo (Tree Star, Inc).

Expression and purification of recombinant Rv0500A

The rv0500A open reading frame from CDC1551 was cloned into pET-28a (Novagen) to construct an in-frame N-terminal 6x-His tag fusion. A sequence verified construct was then transformed into E. coli BL-21 (DE3). For expression, a single transformant colony from an LB plate containing 50 μg/ml kanamycin was picked and grown overnight at 37°C on a roller drum in 2.5 ml of LB broth + 50 μg/ml kanamycin. 1 L of 2YT (5 g NaCl, 10 g yeast extract, and 15 g tryptone per liter) with 50 μg/ml kanamycin was subsequently inoculated with 2 ml of the overnight culture and grown shaking at 37°C to an OD600 of 0.75. To induce protein expression, 1 mM isopropyl-β-D-1-thiogalactopyranoside (IPTG) was added, and the culture grown overnight, shaking, at 18°C. Induced culture was pelleted the next day and resuspended in 25 ml lysis buffer (500 mM NaCl, 50 mM Tris pH 7.5, 15 mM imidazole, 10% glycerol). The resuspended cells were flash frozen in liquid nitrogen, thawed, and lysed via sonication. The insoluble fraction was pelleted and the cleared lysate mixed with 1 ml of Ni-NTA agarose (Macherey-Nagel) and incubated overnight at 4°C on a nutator. Purified protein was eluted the next day using high-imidazole buffer (500 mM NaCl, 50 mM Tris pH 7.5, 200 mM imidazole, 10% glycerol) (elution repeated 8 times in total). Samples were run on a 20% SDS-PAGE gel, visualized with Coomassie Brilliant Blue R-250 (Bio-Rad) staining, and imaged using the 700 nm channel of an Odyssey CLx imaging system (LI-COR). Protein concentration was quantified using a Bradford assay (Bio-Rad).

Electrophoretic mobility shift assays

To assess DNA binding of Rv0500A, promoter regions for rv2390c (full length—704 bp; 5’ section—403 bp; 3’ section—301 bp) and kdpF (754 bp) were amplified using IRDye 700 labeled primers (Integrated DNA Technologies) and the PCR products purified using a QIAquick PCR purification kit (Qiagen). Indicated amounts of purified His-Rv0500A were mixed with no more than 40 fmoles of DNA in EMSA buffer (20 mM Tris-HCl, pH 8, 50 mM KCl, 2 mM MgCl2, 5% glycerol, 0.5 mM EDTA, 1 mM DTT, 0.05% Nonidet P-40, 25 μg/ml salmon sperm DNA [65]) in 11 μl final volume reactions. After incubation at room temperature for 20 minutes, the reactions were run on a non-denaturing 8% Tris-glycine gel in HEPES-imidazole buffer (35 mM HEPES, 43 mM imidazole). The gel was then imaged using the 700 nm channel of an Odyssey CLx imaging system (LI-COR).

Intrabacterial pH assay

Mtb grown to mid-log phase in standard 7H9 broth, pH 7, was pelleted and resuspended to OD600 = 0.6 in 10 ml of PBS (1.54 mM KH2PO4, 2.71 mM Na2HPO4, 155 mM NaCl, pH 7.3) containing 0.05% Tween 80 and 10 μM 5′-chloromethylfluorescein diacetate (Invitrogen) for 1 hour, protected from light. Bacteria were washed twice in their respective buffer type, before resuspension to OD600 = 1.2 in 500 μl of appropriate buffer (PBS, pH 7.3 or pH 5.7; K+-free PBS, pH 7.3 or pH 5.7). To generate K+-free PBS, NaH2PO4 was substituted for KH2PO4. For control samples, 10 μM of the ionophore nigericin was added. 100 μl samples were transferred to a 96-well clear bottom black plate (Corning Costar), with each condition read in triplicate. After equilibration, top read fluorescence at Ex. 450/10 nm, Em. 520/10 nm, and Ex. 490/10 nm, Em. 520/10 nm, was measured using a Biotek Synergy Neo2 microplate reader. The ratio of fluorescence signal at Ex. 490 nm, Em. 520 nm, versus that at Ex. 450 nm, Em. 520 nm, was used to determine relative intrabacterial pH. Data were normalized as a percentage of the fluorescence ratios observed in PBS, pH 7.3, for a given strain [52].

Bacterial membrane potential assay

Mtb grown to mid-log phase were resuspended to OD600 = 0.6 in (i) 7H9, pH 7, (ii) 7H9, pH 5.7, or (iii) K+-free 7H9, pH 7, with each containing 0.5 mg/l rhodamine 123 (Sigma) [53]. 50 μM carbonyl cyanide m-chlorophenylhydrazone (Sigma) was added for control samples. 150 μl quadruplicate aliquots of the bacterial suspensions were then transferred to a 96-well clear bottom black plate. Fluorescence decay was tracked every 10 minutes for 4 hours with a Biotek Synergy Neo2 microplate reader (bottom read Ex. 485/10 nm, Em. 527/10 nm), and normalized to initial probe fluorescence for each strain and condition.

Macrophage culture and infections

C57BL/6J wild type and gp91phox-/- mice (Jackson Laboratories) were used for isolation of bone marrow-derived macrophages. Cells were maintained in DMEM supplemented with 10% FBS, 15% L-cell conditioned media, 2 mM L-glutamine, 1 mM sodium pyruvate, and penicillin/streptomycin as needed, in a 37°C incubator at 5% CO2. Macrophage infections with Mtb were performed as previously described [2, 37]. For CFU enumeration, macrophages were lysed with water containing 0.01% sodium dodecyl sulfate. The strain expressing kdpF’::GFP was pre-induced for 6 days in K+-free 7H9, pH 7, prior to infection as needed.

Confocal immunofluorescence microscopy

Fixed Mtb-infected macrophages were stained with DAPI and Alexa Fluor 647 phalloidin (Invitrogen) for visualization of nuclei and F-actin respectively. Stained samples were mounted with ProLong Diamond antifade, and images acquired with Leica LAS X software using a Leica SP8 confocal laser scanning microscope, with 0.5 μm z-steps. 3D reconstruction and image analyses were carried out with Volocity software (PerkinElmer) as previously described [2, 66, 67].

Generation of K+ beads

K+ sensor beads were generated by first covalently linking human IgG (Sigma) and fatty acid-free bovine serum albumin (Sigma) to 12.5 mg of carboxylated, 3 μm silica beads (Kisker Biotech) as previously described [2, 68]. Beads were then washed once with coupling buffer (0.1 M sodium borate, pH 8.0), and twice with PBS. 20 mg of EDC (Sigma) and 25 μg of Asante Potassium Green 4, TMA+ salt (TEFLabs) were added to the beads in 1 ml of PBS, and the mixture incubated with agitation for 2 hours at room temperature, protected from light. APG4 beads were washed three times with PBS, before resuspension in 1 ml of coupling buffer containing 25 μg of Alexa Fluor 594-SE (Invitrogen), and incubation with agitation for an additional 1 hour at room temperature, protected from light. APG4/AF594 beads were washed twice with coupling buffer, and once with PBS, before final resuspension in 500 μl of PBS.

K+ bead assays

Induction of APG4 fluorescence by K+ was tested by placing APG4/AF594 beads in assay buffer (1.54 mM NaH2PO4, 2.71 mM Na2HPO4, 157.87 mM NaCl, 5 mM dextrose, 1 mM CaCl2, 0.5 mM MgCl2) supplemented with specified concentrations of K+ gluconate, in a 96-well clear bottom black plate. Na+ gluconate supplementation was used for Na+ response tests. For tests with [Na+] less than 157.87 mM, NaCl was excluded from the assay buffer. Tests for response to pH was conducted in assay buffer with 100 mM Bis-Tris added, and pH adjusted with HCl. Each condition was tested in quadruplicate, and bottom reads of Ex. 510 nm/Em. 540 nm (APG4) and Ex. 590 nm/Em. 617 nm (AF594) taken after equilibration with a Biotek Synergy H1 microplate reader.

For intraphagosomal K+ bead assays, primary murine bone marrow-derived macrophages (2x105/well) were seeded in a 96-well clear bottom black plate. Where needed, 100 U/ml IFNγ (PeproTech) and 10 ng/ml LPS (List Biological Laboratories) were used for activation of macrophages. 100 nM concanamycin A (AdipoGen Life Sciences) was added to the media where indicated. Macrophages were washed three times with pre-warmed assay buffer, before addition of APG4/AF594 beads (~2–5 beads/macrophage). A Biotek Synergy H1 microplate reader was used for fluorescence tracking, with four-six replicate wells/condition and bottom reads taken every two minutes for four hours. Temperature was maintained at 37°C throughout the assay.

Mouse Mtb infections

C57BL/6J wild type mice (Jackson Laboratories) were infected intranasally with 103 CFUs of Mtb (35 μl), under light anesthesia with 2% isoflurane. After sacrifice with CO2, the left lobe and accessory right lobe were homogenized in PBS containing 0.05% Tween 80 and serial dilutions plated on 7H10 agar plates containing 100 μg/ml cycloheximide for CFU determination. The remaining three right lobes were fixed in 4% PFA in PBS, and used for histology examination via standard hematoxylin and eosin (H&E) staining (Tufts Comparative Pathology Services). H&E stained slides were imaged on a Nikon Eclipse E400 equipped with a SPOT Insight color digital camera.

Accession number

RNA sequencing data has been deposited in the NCBI GEO database (GSE120725).

The K+ response regulon is specific and not triggered by changes in [Na+].

qRT-PCR of gene expression in WT Mtb grown in Na+-free 7H9, pH 7, compared to 7H9 with standard [Na+], pH 7, for 4 hours. Data are shown as means ± SD from 3 technical replicates, representative of 2 independent experiments.

(TIF)

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rv2390c’::GFP does not respond to low [K+].

CDC1551(rv2390c’::GFP) was grown in standard 7H9 broth, pH 7.0 ± 250 mM NaCl, or in K+-free 7H9 broth, pH 7.0, supplemented with 0.01 mM KCl. Samples were taken at indicated time points, fixed, and GFP induction analyzed by FACS. Data are shown as means ± SD from 3 independent experiments.

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Expression and purification of recombinant Rv0500A.

Recombinant N-terminally 6x-His-tagged Rv0500A was expressed and purified from E. coli BL-21 (DE3). Coomassie Brilliant Blue R-250 stained gel shows the cleared lysate sample and the eluate fraction used in the EMSA assays.

(TIF)

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Inhibition of H+-ATPase activity significantly diminishes intraphagosomal [K+] increase.

APG4/AF594 beads were added to resting murine bone marrow-derived macrophages (MØ) in the presence of either DMSO (carrier control) or 100 nM concanamycin A, and fluorescence tracked with a microplate reader over time. Sensor beads were also added to wells containing only media, with no macrophages (“beads only, no MØs”). Data are shown as means ± SD from 4–6 wells, representative of 3 independent experiments.

(TIF)

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Mtb ΔceoBC mutant is more sensitive to low environmental [K+].

WT, ΔceoBC, or ceoBC* (complemented mutant) Mtb carrying the K+ responsive kdpF’::GFP reporter were grown in standard 7H9 broth, pH 7.0, or in K+-free 7H9 broth, pH 7.0, supplemented with 0.2 mM KCl for 9 days. GFP signal in fixed samples was measured by FACS, with fold signal induction compared to the corresponding strain grown in pH 7 control media. Data are shown as means ± SD from 3 independent experiments. p-values were obtained with an unpaired t-test, * p<0.05, ** p<0.01.

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Genes upregulated >2-fold, p<0.05, after 4 hours exposure to K+-free 7H9.

(XLSX)

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Genes downregulated >2-fold, p<0.05, after 4 hours exposure to K+-free 7H9.

(XLSX)

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