Search tips
Search criteria 


Logo of plosonePLoS OneView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS One. 2010; 5(7): e11058.
Published online 2010 July 6. doi:  10.1371/journal.pone.0011058
PMCID: PMC2897852

Mycobacterium tuberculosis ClpX Interacts with FtsZ and Interferes with FtsZ Assembly

David M. Ojcius, Editor


FtsZ assembly at the midcell division site in the form of a Z-ring is crucial for initiation of the cell division process in eubacteria. It is largely unknown how this process is regulated in the human pathogen Mycobacterium tuberculosis. Here we show that the expression of clpX was upregulated upon macrophage infection and exposure to cephalexin antibiotic, the conditions where FtsZ-ring assembly is delayed. Independently, we show using pull-down, solid-phase binding, bacterial two-hybrid and mycobacterial protein fragment complementation assays, that M. tuberculosis FtsZ interacts with ClpX, the substrate recognition domain of the ClpXP protease. Incubation of FtsZ with ClpX increased the critical concentration of GTP-dependent polymerization of FtsZ. Immunoblotting revealed that the intracellular ratio of ClpX to FtsZ in wild type M. tuberculosis is approximately 1[ratio]2. Overproduction of ClpX increased cell length and modulated the localization of FtsZ at midcell sites; however, intracellular FtsZ levels were unaffected. A ClpX-CFP fusion protein localized to the cell poles and midcell sites and colocalized with the FtsZ-YFP protein. ClpX also interacted with FtsZ mutant proteins defective for binding to and hydrolyzing GTP and possibly for interactions with other proteins. Taken together, our results suggest that M. tuberculosis ClpX interacts stoichiometrically with FtsZ protomers, independent of its nucleotide-bound state and negatively regulates FtsZ activities, hence cell division.


Mycobacterium tuberculosis, the causative agent of tuberculosis, has spread dramatically worldwide, and recent years have seen not only an increase in the number of multidrug-resistant strains but also the emergence of extensively drug-resistant M. tuberculosis [1], [2]. Eradication of M. tuberculosis infection necessitates the development of novel drugs targeted to hitherto unidentified metabolic processes and pathways of the pathogen, and FtsZ catalyzed cell division is one such process. FtsZ, the homolog of eukaryotic tubulin, is a highly conserved protein and plays a central and essential role in initiation of the cell division process [3], [4]. M. tuberculosis FtsZ, like its bacterial counterparts, exhibits GTP binding and hydrolysis activities and localizes to the midcell division site in the form of a Z-ring [5], [6]. FtsZ-ring assembly in M. tuberculosis is delayed under several conditions relevant to its growth; two of these are growth in macrophages and exposure to cephalexin [5]. The identities of the regulators affecting Z-ring assembly and the cell division process in M. tuberculosis, however, are largely unknown. Identification and characterization of such regulators would improve our understanding of the cell division process in M. tuberculosis.

Elegant genetic and cell biological studies carried out in other bacteria indicate that Z-ring assembly is regulated by the counterbalancing activities of positive and negative regulators that directly or indirectly modulate FtsZ activities (reviewed in [4]). These regulators include FtsA, ZipA, ZapA, Slm, SulA, YneA, Noc, EzrA, CrgA and ClpX; however, not all of these regulators are conserved in all bacteria (reviewed in [7]). The M. tuberculosis genome appears to lack most of the known regulators, except for the genes encoding ClpX, CrgA and a YneA-like protein, ChiZ [5], [8]. We recently showed that ChiZ is a DNA damage-inducible protein that shows peptidoglycan hydrolysis activity and functions to regulate Z-ring assembly and cell division in M. tuberculosis [5]. It is unknown if ClpX serves as a potential cell division regulator in M. tuberculosis. ClpX, the substrate recognition part of the ClpXP protease, is well conserved in prokaryotes [9], [10], [11]. In the ClpXP complex, ClpX is present in a hexameric ring and is attached to the twin-stacked heptameric ClpP rings via the protease interface surface (reviewed [9]). ClpX belongs to the AAA ATPase family and contains the characteristic Walker A and Walker B motifs required for ATP binding and hydrolysis, respectively [12], [13], [14]. By itself, ClpX works as a chaperone, whereas in association with the ClpP protease, it is believed to eliminate misfolded, aggregated and dysfunctional protein targets [9]. It is interesting to note that, unlike Escherichia coli, Caulobacter crescentus and B. subtilis, the M. tuberculosis genome appears to contain one clpX and two clpP genes, designated as clpP1 and clpP2 [15]. On the other hand, the presence of clpP1 and clpP2 is common to members of Actinomycetales, including Mycobacterium spp. [16], [17].

Recent studies with C. crescentus and B. subtilis revealed that ClpX or ClpXP complex functions as a regulator of cell division, although the mechanisms by which it affects cell division appear to vary in the two species. Furthermore, two independent studies with E. coli ClpX led to two different conclusions (see below). In the case of Gram negative and alpha-proteobacterium C. crescentus, the ClpXP protease regulates the transcription of cell division genes via degradation of the master cell cycle regulator, CtrA [11], [18]. In E. coli, another Gram negative bacterium, Camberg et al [19] reported that ClpXP regulates cell division by degrading FtsZ in an ATP-dependent manner, thereby affecting the equilibrium between monomeric and polymeric FtsZ. In contrast, single molecule analysis study with high-speed atomic force microscopy revealed that ClpX regulates dynamics of FtsZ assembly by blocking the reassembly of FtsZ in an ATP independent manner and that ClpXP protease shows only a weak protease activity against FtsZ in the presence of either GTP or GDP [20]. These results, which are inconsistent with the findings of Camberg et al [19], suggest that the contribution of FtsZ unfolding by ClpX is negligible as compared to its role in the inhibition of FtsZ assembly [20]. Nevertheless, the observed intracellular levels of ClpX and FtsZ in E. coli appear to be 600 and 15,000 molecules per cell, respectively [21], [22] leading to a suggestion that ClpXP could play a catalytic role in regulating FtsZ assembly. It is pertinent to note that the proteomic studies with E. coli lysates utilizing the ClpXPtrap protocol identified FtsZEcoli as one of the ~60 proteins associated with ClpXPEcoli [23]. In B. subtilis, ClpX inhibits FtsZ assembly in vivo and interferes with the FtsZ polymerization activity in vitro independent of its ATPase activity [24], [25]. Thus the above divergent results in different organisms necessitate the evaluation of the role of ClpX in cell division in other bacteria including the human pathogen, M. tuberculosis.

To begin evaluating the roles of ClpX, if any, in M. tuberculosis cell division, we characterized interactions of ClpX with FtsZ in vivo and in vitro. We show that clpX expression is elevated during intracellular growth and upon cephalexin treatment, two of the conditions known to delay FtsZ ring assembly [5]. Independently, we show that ClpX functions to regulate FtsZ activity in vitro and FtsZ assembly in vivo by interacting with FtsZ and that both proteins colocalize at the cell division site. Our results are consistent with a model that ClpX activity is one of the factors responsible for the regulation of M. tuberculosis Z-ring assembly during intracellular growth and that ClpX action on FtsZ and cell division is possibly conserved in eubacteria.


clpX expression is upregulated during intracellular growth

To begin evaluating the role of ClpX in FtsZ catalyzed cell division process in M. tuberculosis, we first examined clpX expression under select growth conditions where M. tuberculosis FtsZ assembly is shown to be modulated, i.e., growth in macrophages and exposure to antibiotics [5], [26]. Accordingly, we determined clpX expression relative to the housekeeping gene 16S rRNA by qRT-PCR during intramacrophage growth and upon exposure to cephalexin antibiotic (Fig. 1). Our results indicated that clpX expression was upregulated during intramacrophage growth and upon exposure to cephalexin (Fig. 1). Since M. tuberculosis cells growing in macrophages and those exposed to cephalexin antibiotic are deficient in FtsZ assembly [5], [26], we examined if ClpX is involved in regulating FtsZ assembly and cell division in M. tuberculosis.

Figure 1
clpX expression in M. tuberculosis.

ClpX inhibits the GTP-dependent FtsZ polymerization activity

The 90° right angle light scatter assay is a widely used method to measure the GTP-dependent polymerization of FtsZ [27]. To examine whether ClpX interferes with FtsZ polymerization activity, purified FtsZ (5.4 µM) was incubated without or with ClpX (2 µM) at 30°C and polymerization was initiated with 1 mM GTP. Since ClpX is thought to possess ATPase activity, 1 mM ATP was included in all polymerization reactions. Consistent with our earlier data, the presence of ATP had no effect on GTP-dependent FtsZ polymerization (data not shown; [28]). In the presence of ClpX, an ~35% reduction in GTP-dependent FtsZ assembly was noted (Fig. 2A). Control experiments with RecA, an ATPase (reviewed in [29]), (Supplementary data Fig. S1) or BSA (data not shown) had no effect on FtsZ polymerization. These results suggest that M. tuberculosis ClpX interferes with FtsZ polymerization.

Figure 2
ClpX inhibits the assembly of FtsZ.

To gain insights into the mechanism by which ClpX inhibits FtsZ assembly, increasing concentrations of FtsZ were incubated with a fixed concentration of ClpX (2 µM) and sedimentation assays performed to determine the extent of FtsZ polymerization (supplementary Fig. S2, panel B). A control experiment lacking ClpX was also performed (supplementary Fig. S2, panel A). As can be seen, in the absence of ClpX, FtsZ polymers were present in the pellet at 1 µM and beyond, (supplementary Fig. S2, panel A, compare lanes S with P). Determination of the amount of FtsZ polymer in the pellet as a function of FtsZ concentration revealed that the critical concentration for FtsZ polymerization was ~1 µM. In the presence of 2 µM ClpX, the amount of FtsZ in the pellet at all protein concentrations was decreased (supplementary Fig. S2, panel B). Furthermore, densitometric determination of the FtsZ levels in the supernatant and pellet fractions revealed that irrespective of the concentration of FtsZ used, the amount of FtsZ in the supernatant was the same, and the critical concentration for FtsZ polymerization was increased to ~2.4 µM (Fig. 2B). Owing to the difficulty in purifying higher than ~8 µM ClpX, these experiments could not be performed at higher concentrations of ClpX. Nonetheless, the above data indicate a stoichiometric association between the FtsZ and ClpX molecules and suggest that ClpX modulates FtsZ assembly by sequestration.

In the above experiments, ClpX was added along with FtsZ. Next, we added ClpX to preformed FtsZ polymers (supplementary Fig. S3). Even under these conditions, unlike with the buffer control, FtsZ was present in the supernatant (supplementary Fig. S3, see reactions 4 and 5, and compare with 2 and 3). Together, these experiments indicate that ClpX interferes with FtsZ polymerization regardless of whether it is added before the initiation of polymerization or after the formation of FtsZ polymers.

GTPase activity of FtsZ is not needed for inhibition of polymerization by ClpX

We next examined the inhibition of FtsZTB assembly by ClpX in the presence of GTP or GMPCPP, a non-hydrolyzable analog of GTP (Fig. 2C) [30], [31]. FtsZTB polymerization occurred in the presence of GMPCPP, as with GTP. Addition of ClpX interfered with the assembly of FtsZTB in the presence GMPCPP (Fig. 2C). These data indicate that ClpX inhibition of FtsZ assembly is independent of the GTP hydrolysis activity of FtsZ.

FtsZ interacts with ClpX

The above data are consistent with the idea that the ClpX-mediated interference with M. tuberculosis FtsZ polymerization activity involves direct physical interaction between the two proteins in M. tuberculosis. Although M. tuberculosis FtsZ exhibits GTP binding and hydrolysis activities like other bacterial FtsZ counterparts, notable differences in these properties have been observed [28], [32]. Furthermore, as reviewed, the M. tuberculosis genome lacks several identifiable homologs of known proteins of the bacterial cell division machinery [5], [33], [34]. Hence, we evaluated physical and functional interactions between the ClpX and FtsZ proteins of M. tuberculosis using a variety of in vitro and in vivo assays.

In vitro: Pull-down assay shows that FtsZ copurifies with His-ClpX

A pull-down assay was performed to evaluate interactions between the ClpX and FtsZ proteins. Equimolar amounts of purified recombinant His-ClpX protein (molarity based on monomer concentration) and a tag-free FtsZ protein created by cleaving the polyhistidine tag were mixed and applied to Ni-NTA resin. Following washing, bound proteins were eluted with imidazole and detected by immunoblotting using anti-ClpXBS and anti-FtsZ antibodies. Both His-FtsZ and tag-free FtsZ showed distinct mobilities on NuPAGE gels (Fig. 3A). As can be seen, the elution fraction containing ClpX also contained FtsZ (Fig. 3B). Some FtsZ was also found in the flow-through and early wash fractions (data not shown), indicating that not all of the FtsZ was complexed with ClpX. In a reverse experiment, we were able to pull-down MBP-ClpX with His-FtsZ on Ni-NTA resin (data not shown). Salt concentrations of 0.2 M weakened the ClpX-FtsZ complexes and those of 0.5 M nearly abolished the interaction (Supplementary Fig. S4, panel A). ClpX-FtsZ complexes were also isolated when E. coli lysates containing the His-ClpX and FtsZ-S-tag were processed on nickel-affinity columns (Supplementary Fig. S4, panel B). Control experiments with lysates containing recombinant N-terminal FtsQ protein (amino acid 1–100; Table S2), His-FtsQN100, and FtsZ did not recover FtsZ in the fractions containing His-FtsQN100 (Fig. 3C), indicating that the observed interaction between ClpX and FtsZ is specific.

Figure 3
FtsZ interacts with ClpX in vitro.

In vitro: Solid-phase binding assay confirms ClpX-FtsZ interactions

Next, a solid-phase binding assay was carried out to further confirm interactions between FtsZ and ClpX. In this assay, ClpX or BSA immobilized in the wells of a microtiter plate was incubated with increasing concentrations of FtsZ. Following washing, the bound FtsZ protein was immunodetected and quantified by ELISA. As can be seen, FtsZ bound to the ClpX-coated wells but not to the wells coated with BSA (Fig. 3D).

In vivo: BACTH assays reveal interactions between ClpX and FtsZ

Next, BACTH assays were performed to evaluate in vivo interactions between ClpX and FtsZ [35]. In these assays, ftsZ and clpX genes were cloned as fusions to the T25 or T18 fragments of adenylate cyclase in two separate vectors and transformed into the E. coli reporter strain, BTH101 [35]. Functional complementation of adenylate cyclase activity due to interactions between the partners leads to cAMP production and subsequent transcription of the lac reporter gene, which gives a distinct color to colonies growing on indicator agar plates. The strength of the interaction was also measured by assaying for the β-galactosidase activity. As expected, the gcn4-gcn4 positive control strain showed high β-galactosidase activity (Fig. 4A). Transformants expressing ftsZ or clpX from both vectors were also red, indicating self-interactions in these proteins (Fig. 4A). Similarly, the transformants expressing ftsZ and clpX were also red, but not when clpX or ftsZ was expressed with the control plasmid (see Fig. 4A). The amount of β-galactosidase produced with the transformants expressing ftsZ and clpX was comparable to the gcn4-gcn4 positive control and also to those expressing clpX or ftsZ from both vectors indicating that the interaction between ClpX and FtsZ is strong (Fig. 4A). These results were consistently obtained with any combination of vectors used to express the clpX and ftsZ genes (Fig. 4A). The specificity of ClpX-FtsZ interaction was indicated by the lack of interaction between ClpX and FtsQ and also between FtsZ and FtsI (see [36]) (Fig. 4A). Interactions between ClpXΔN200, lacking the N-terminal Zinc-binding, ATP binding and ATP hydrolysis domains, and FtsZ appeared to be weak, as the amount of β-galactosidase produced was just above the background. These data suggest that the N-terminal region of ClpX is important for optimal interactions with FtsZ (supplementary Fig. S5, panel A; Table S2). Together, the above results validate the in vitro data showing interactions between the ClpX and FtsZ proteins.

Figure 4
FtsZ interacts with ClpX in vivo.

In vivo: M-PFC assay confirms ClpX and FtsZ interactions

We next examined the interactions between ClpX and FtsZ proteins in their native environment using the M-PFC assay [37]. This assay scores for trimethoprim (Trim) resistance due to the regeneration of functional murine dihydrofolate reductase (mDHFR) activity from two independent mDHFR protein fragment domains fused to two potential protein interaction partners. The strength of interaction is measured by monitoring the reduction of alamar blue in growth media containing Trim [37]. Accordingly, we fused full-length clpX and ftsZ to the 3′ or 5′ end of murine dhfr fragments 1–2 and 3 in bait and prey vectors, respectively, and expressed them from the tetracycline-inducible promoter in M. smegmatis (see methodology section and Table S2). The recombinant strains expressing Ptet::clpX-dhfr1,2 and Ptet::ftsZ-dhfr3 showed resistance to Trim (Fig. 4B), similar to those expressing ftsZ/ftsZ or gcn4/gcn4, the two positive controls. Negative control transformants expressing gcn4 and clpX did not show any growth on Trim plates (Fig. 4B). Evaluation of the extent of alamar blue reduction confirmed these results (Fig. 4C). Transformants expressing Ptet::clpXΔN200-dhfr1,2 and Ptet::ftsZ-dhfr3 did not grow on Trim plates (Supplementary Fig. S5, panel B) corroborating the conclusion from BACTH data that the N-terminal 200 amino acids of ClpX are needed for interaction with FtsZ.

ClpX interaction with mutant FtsZ proteins

As reviewed, FtsZ binds GTP and exhibits GTP-dependent polymerization and GTP hydrolysis activities [28], [32]. FtsZ also interacts with FtsW in vitro [38] and in vivo [34]. The amino acid residues in FtsZ important for these activities have been identified. For example, FtsZG103S is defective in binding to GTP; hence, is also defective in GTP hydrolysis. FtsZD210G, on the other hand, is proficient in GTP binding, but is defective in GTP hydrolysis [28]. FtsZD374-76A is defective in its interactions with FtsW [34]. FtsZΔC21 lacks 21 amino acids from the C-terminus, a region believed to be critical for interactions of FtsZ with other cell division proteins [38], [39], [40], [41]. To investigate if ClpX interacts with FtsZ mutants defective in the above-described activities, we purified FtsZG103S, FtsZD210G, FtsZD374-76A and FtsZΔC21 recombinant proteins and investigated their interaction using pull-down and BACTH assays [34], [35], [38]. Pull-down assays with mixtures of equimolar amounts of His-ClpX and various FtsZ mutant proteins followed by immunoblotting confirmed the presence of FtsZ in fractions containing ClpX (Fig. 5A). The BACTH assay confirmed these data (Fig. 5B, 5C). ClpX also inhibited the assembly of FtsZΔC21 (Fig. 5D). These data suggest that ClpX is capable of interacting with monomeric or polymeric FtsZ and that the C-terminal region of FtsZ is not required for this interaction.

Figure 5
ClpX interacts with various FtsZ mutants.

Overexpression of clpX inhibits Z-ring assembly and reduces M. tuberculosis viability

Saturated transposon mutagenesis studies have indicated that clpX is an essential gene, like the ftsH protease [42]. While it is still possible that clpX is not essential in M. tuberculosis, saturation transposon screens are comprehensive. We would like to note that our innumerable attempts to make a knock-out ftsH, another protease shown by transposon mutagenesis to be essential, by homologous recombination were unsuccessful (Chauhan and Rajagopalan, unpublished data). Therefore, to evaluate the consequences of the interaction of ClpX with FtsZ in vivo, we created M. tuberculosis strains expressing altered levels of ClpX from the inducible tetracycline promoter and characterized them with respect to growth, viability and Z-ring structures. Quantitative immunoblotting determined the intracellular levels of ClpX monomers in exponential phase cultures of WT M. tuberculosis to be ~14,000 molecules per cell (Fig. 6A, see legend for details). Under the same conditions, FtsZ levels were previously determined to be ~30,000 molecules per cell (12), and this makes the approximate ratio of ClpX (monomeric) to FtsZ 1[ratio]2. Immunoblotting also revealed that the ClpX levels were elevated by ~six-fold in the presence of anhydrotetracycline in the sense clpX strain (pRD23, Table S2; inset in Fig. 6B). The low level of the ClpX signal in the antisense strain (asClpX) made it difficult to accurately determine the reduction in ClpX levels in this strain (data not shown). As an alternative, we evaluated clpX transcript expression by qRT-PCR (supplementary Fig. S6). The clpX transcript expression relative to the housekeeping gene 16S rRNA was decreased by 12-fold in the asClpX strain (supplementary Fig. S6).

Figure 6
Overproduction of ClpX delays growth and cell division of M. tuberculosis.

We next examined if intracellular levels of FtsZ were altered in cells producing altered levels of ClpX. The FtsZ levels were neither decreased under ClpX overproduction condition nor increased under ClpX underproduction condition, i.e. in asClpX strain (supplementary Fig. S7, panels A and B). Together, these results suggest that altered levels of ClpX do not affect intracellular M. tuberculosis FtsZ levels. We also found that M. tuberculosis sense and antisense clpX strains showed a moderate reduction in growth (Fig. 6B) and viability (supplementary Fig. S8). These defects can possibly be attributed to interruptions in the ClpX chaperone and protein degradation functions due to reduction in ClpX levels.

The merodiploids overexpressing clpX were elongated, with an ~50% increase in cell length (3.3 µm ±0.25) as compared to WT (2.2 µm ±0.58; Fig. 6C, compare brightfield panels WT and ClpX). Visualization of nucleoid staining with DAPI revealed elongated cells with multiple nucleoids (Fig. 6C, see arrows in ClpX panels). In contrast, the WT cells had one or two distinct nucleoids per cell (Fig. 6C, WT panels). A decrease in ClpX levels caused only a modest 7% increase in cell length (2.36 µm ±0.11), and the DAPI staining patterns were similar to WT (Fig. 6C, asClpX panels).

To determine whether the observed morphological changes associated with ClpX overproduction were due to defects in FtsZ ring assembly, we created an M. tuberculosis strain expressing Ptet::ftsZ-gfp and Ptet::clpX, visualized FtsZ structures and compared the results with the control strain expressing Ptet::ftsZ-gfp. Incubation of the control strain with 5 ng of anhydrotetracycline for 24 h revealed distinct bright FtsZ-structures at the midcell position (Fig. 7D, see arrow 1) and in some cases, at the cell poles (Fig. 7D, arrow 2). The midcell rings accounted for 16.8±1.4% of cells (n = 627). The polar FtsZ localization, believed to be a remnant from the previous cell division, accounted for approximately 6.5% of cells. These results are consistent with our earlier published data [26]. In contrast, M. tuberculosis cells expressing Ptet::ftsZ-gfp and Ptet::clpX were elongated, with an average cell length of 5.5±1.0 µms (Fig. 7, compare panel A with C). Unlike the WT cells (2.1±0.6 µms), many elongated cells were devoid of bright Z-rings and had diffuse fluorescence along the entire cell length. Approximately 10.8±2.2% of cells had less-fluorescent midcell Z-rings, which tended to bleach quickly (see discussion). Polar FtsZ structures were rarely present (Fig. 7, panel F), and some elongated cells had aberrant FtsZ-GFP localization (Fig. 7, panel F, see arrowhead). The average length of FtsZ-GFP ring containing cells increased by 52% under ClpX overproduction conditions. Increased cell length and diffuse midcell Z-rings are consistent with the idea that increased ClpX levels delay FtsZ assembly and cell division in M. tuberculosis.

Figure 7
Altered ClpX levels affect FtsZ ring formation in M. tuberculosis.

The antisense clpX cells showed FtsZ structures at midcell sites and cell poles, as in the WT strain, but these structures were less vibrant (Fig. 7, asClpX panels). Since all strains were grown and processed under similar conditions, we believe that the diffuse fluorescence of FtsZ-GFP rings in asClpX strain is not an artifact of microscopy. Given that clpX is an essential gene [42], lowered ClpX levels might therefore affect the activities of other proteins and/or other potential regulators of cell division.

ClpX-CFP localizes to the cell poles and to midcell sites and colocalizes with FtsZ

Visualization of fewer and fainter FtsZ-structures under ClpX overproduction conditions suggested that fewer FtsZ molecules were in the midcell Z-ring. This could be due to sequestration of FtsZ protomers by ClpX thereby limiting the available pools of FtsZ for polymerization. Alternatively, ClpX association with FtsZ in the midcell Z-rings could lead to the latter's disassembly. Both possibilities are not mutually exclusive. To address the latter possibility, we attempted to visualize ClpX structures by creating an M. tuberculosis strain expressing Ptet::clpX-cfp and determining whether ClpX colocalizes with FtsZ. The ClpX-CFP structures in M. tuberculosis were less distinct and generally more diffuse (Fig. 8, panel B). It is presumed that the fluorescence quenching is due to the paraformaldehyde fixation step required in processing samples with the virulent strain. To visualize ClpX without paraformaldehyde fixation, we expressed Ptet::clpXTB-cfp in M. smegmatis, a rapidly growing and nonpathogenic mycobacterial member. Visualization of ClpX-CFP in M. smegmatis revealed distinct localization at the cell poles in the majority of cells and at midcell sites in a small fraction of cells (Fig. 8A). When quantified, these structures corresponded to 82.5±6.5% at the cell poles and 11±2% at midcell sites (n = 124). Next, to address whether ClpX-CFP colocalizes with FtsZ, we transformed Pami::ftsZ-yfp into the M. smegmatis strain expressing Ptet::clpX-cfp and visualized ClpX and FtsZ following a 1-h induction with 5 ng of anhydrotetracycline and 0.2% acetamide. As expected, FtsZ-YFP structures were evident at midcell sites and poles (Fig. 8C, see panel FtsZ-YFP), similar to our earlier published data [34]. ClpX-CFP showed similar localization (Fig. 8C, see panel ClpX-CFP). The FtsZ-YFP structures were faint and tended to bleach easily. Even with this limitation, we were able to see a colocalization pattern (see Fig. 8, panel C Merge). ClpX-FtsZ colocalization was noted at the cell poles in 12±2.8% of cells and at midcell sites in 3.5±2.1% of cells (n = 110).

Figure 8
Localization of ClpX and FtsZ proteins in M. smegmatis and M. tuberculosis.


The results presented in this study show that M. tuberculosis ClpX interacts with FtsZ and a possible consequence of these interactions is modulation of Z-ring assembly at midcell sites in vivo and interference with GTP-dependent FtsZ polymerization activity in vitro (Figs. 7, ,88 and and2).2). The critical concentration of FtsZ polymerization is increased in the presence of ClpX (Fig. 2B). The intracellular levels of FtsZ are, however, unaffected upon ClpX overproduction. These results, combined with the observation that the intracellular ratio of ClpX to FtsZ is 1[ratio]2, are consistent with a notion that in M. tuberculosis ClpX interacts with FtsZ at stoichiometric levels. Such an interaction could lead to sequestration of the available pools of FtsZ required for catalyzing Z-ring assembly and cell division in M. tuberculosis.

FtsZ localization at midcell sites and cell poles and the potential regulators affecting Z-ring assembly have been extensively studied in E. coli, B. subtilis and a handful of other bacteria (reviewed in [7]). In contrast to the situation in other bacteria, only a few proteins affecting Z-ring assembly in M. tuberculosis have been identified. One of these is ChiZ (Rv2719c), a cell wall hydrolase and a negative regulator of cell division [5]. The ChiZ protein has been shown to modulate Z-ring assembly by localizing its activity to midcell sites and cell poles, the same locations where FtsZ is found [5]). The ChiZ protein, however, does not interact with FtsZ; hence, the interference effects are rather indirect. The second protein is FtsW, a bona fide FtsZ-interacting partner [38] hypothesized to function as a positive regulator of Z-ring assembly [34], [38]. Genetic studies indicate that FtsW is required for productive FtsZ ring formation and that FtsW possibly functions to promote and stabilize Z-rings in mycobacteria [34]. More recently, FipA, a FtsZ interacting protein has been shown to be required for sustenance of cell division in M. tuberculosis under oxidative stress conditions [43]. The results presented in this study attest that M. tuberculosis ClpX is a bona fide interaction partner of FtsZ and potentially acts as a negative regulator of Z-ring assembly and cell division. Thus, ClpX joins the list of proteins that regulate Z-ring assembly and cell division in the human pathogen M. tuberculosis.

As reviewed, the modes of action of ClpX or ClpXP in cell division control are distinctly different in different bacterial species. C. crescentus ClpXP indirectly regulates cell division by degrading the CtrA regulator thereby modulating the expression of cell division genes [11], [44], [45]. B. subtilis ClpX inhibits FtsZ polymerization activity in vitro and Z-ring assembly in vivo, independent of the ClpXP protease activity [24], [25]. The physical interaction between the ClpX and FtsZ proteins in B. subtilis, however, was not investigated in these studies. ClpX is an abundant protein in B. subtilis, with 8,400 molecules per cell [46]. Thus, it is likely that ClpX operates at stoichiometric levels in affecting FtsZ activities in B. subtilis. While this work was in progress, two recent reports indicated contrasting roles for E. coli ClpX in cell division. One study concluded that ClpXP operates catalytically to degrade FtsZ polymers and monomers, thereby modulates the equilibrium between free and polymeric FtsZ required for Z-ring assembly in an ATP-dependent manner [19]. The other study reported that E. coli ClpX directly modulates FtsZ polymer dynamics by disassembling FtsZ polymers in an ATP-independent manner [20] and that ClpXP protease activity contributes to a minor role in cell division regulation. Therefore, our studies showing a physical interaction between ClpX and FtsZ (Figs. 35),5), the similar intracellular FtsZ levels in cells producing altered levels of ClpX (supplementary Fig. S7), the modulation of FtsZ polymerization in vitro and Z-ring assembly in vivo (Figs. 2 and and7),7), combined with the finding that the intracellular ratio of ClpX to FtsZ is 1[ratio]2 (Fig. 6A), are consistent with the notion that in M. tuberculosis ClpX interacts with FtsZ and possibly interferes with Z-ring assembly by sequestering the available intracellular pools of FtsZ. While this reasoning assumes that overproduction of ClpX in vivo could lead to cell division arrest and extensive filamenation, in reality this might not happen (see below). For example, our results showed that a 6-fold overproduction of ClpX caused ~50% increase in cell length. While this can be considered modest, it is noteworthy that a 2-fold increase in ClpX in B. subtilis resulted in only a ~20% increase in cell length [25]. ClpX is the substrate recognition part of the ClpXP protease complex. Thus, increased levels of ClpX could promote its interaction not only with FtsZ but also with its other substrates. For example, the ClpXP complex in E. coli is known to associate with ~60 proteins [23]. Therefore, while the in vitro results suggested that FtsZ and ClpX interact stoichiometrically, the extent of in vivo filamentation would likely depend on the ClpX ‘available’ for FtsZ (cell division) inhibition. The observed modulation of Z-ring assembly upon ClpX overproduction was carried out in M. tuberculosis background WT for clpP1 and clpP2. Thus, our data also suggest that ClpX mediated modulation of FtsZ assembly is independent of the presumptive M. tuberculosis ClpXP protease activity as in B. subtilis and possibly in other bacteria.

Our studies with FtsZ mutant proteins, FtsZG103S, defective in binding to GTP and, hence, defective in polymerization [28], FtsZD210G, defective in GTP hydrolysis and, hence, deficient in exhibiting polymer dynamics [47], FtsZD374-76A and FtsZΔC21 which are defective for interactions with FtsW [34], [38], and possibly other proteins, indicate that M. tuberculosis ClpX interacts with FtsZ independent of FtsZ oligomeric state or associations with other proteins. Parallel data showing that ClpX interferes with FtsZ polymerization activity in the presence of the non-hydrolysable GTP analog, GMPCPP [31], reduces the amount of FtsZ polymers formed even when added to preformed FtsZ polymers (Fig. S3) and the colocalization of ClpX-CFP with FtsZ-YFP at midcell Z-rings (Fig. 8) are in partial support of the above conclusions. Together, these results are consistent with a model in which M. tuberculosis ClpX interacts with FtsZ independent of its oligomeric state or associations with other proteins and sequesters FtsZ from engaging in its activities. This line of thinking suggests that ClpX, like SulA of E. coli, inhibits the FtsZ polymerization by a sequestration mechanism [31]. However, unlike ClpX, the E. coli SulA protein does not inhibit FtsZ polymerization in the absence of GTP hydrolysis. The E. coli MinC also requires GTP hydrolysis activity of FtsZ for inhibition of polymer assembly. Since MinC does not affect the GTPase activity of FtsZ it is thought that MinC requires dynamic FtsZ polymers to exert its effect [30].

Our studies raise questions as to when the consequences of FtsZ and ClpX interactions lead to modulation of Z-ring assembly in M. tuberculosis, especially since overproduction of ClpX led to only modest changes in cell length and growth rate (Fig. 6). To answer this question, it is important to recognize that both M. tuberculosis ClpX and FtsZ are relatively abundant proteins and are present at an intracellular ratio of 1[ratio]2. ClpX is a component of the ClpXP protease and could be interacting with other hitherto unrecognized interaction partners, similar to the situation reported in E. coli [23]. Thus, we expect that under normal growth conditions ClpX interactions with FtsZ would not lead to interference of Z-ring assembly in M. tuberculosis. Limited ~6-fold overproduction of ClpX (Fig. 6B inset), however, could impair the optimal intracellular ratio between ClpX and FtsZ. This could in turn interfere with FtsZ activities and affect Z-ring assembly. It is important to note in this regard that ClpX expression is upregulated during intracellular growth and upon exposure to antibiotic stress, the same growth conditions where the intracellular levels of FtsZ are not affected [26]. FtsZ ring assembly is modulated by these conditions, however, and cell division is delayed [26]. The expression of clpX is likely modulated in response to various environmental cues and the induced ClpX possibly functions as a chaperone and as part of the ClpXP protease. We propose that under some circumstances such as growth of M. tuberculosis in macrophages and upon exposure to antibiotic cephalexin, ClpX also modulates FtsZ-ring assembly such that the pathogen can cope with the stress of survival.

M. tuberculosis Z-ring assembly, as in E. coli and B. subtilis [48], [49], is a dynamic process, and the subunits in the FtsZ ring undergo constant turnover [47]. Studies have also indicated that ~30% of the FtsZ protein pool is in the Z-ring, while the remainder is likely to be present as short polymers and monomers [49]. Therefore, it is likely that in M. tuberculosis, ClpX-bound FtsZ monomers are incompatible for polymerization or exchange with the subunits in FtsZ polymers or protofilaments [32], [47], [50]. This, in turn, could limit subunit exchange and prevent productive Z-ring assembly. Although further studies are required to address these issues in detail, our data suggest that ClpX could be one of the factors regulating M. tuberculosis Z-ring assembly during intracellular growth.

We found approximately three times more colocalization of ClpX and FtsZ at the cell poles compared to midcell sites (Fig. 8). However, our data do not rule out a possibility that colocalization of ClpX and FtsZ could also be due to their respective interactions with other proteins. And while colocalization of two proteins is not a direct indication of interaction, these data combined with bacterial two-hybrid and MPFC assays suggest that increased ClpX localization at the cell poles helps to disassemble the remnants of FtsZ polymers from new cell poles and to restrict polar ring formation. It is known that the MinCDE system is critical for targeting FtsZ to midcell sites [3]. The M. tuberculosis genome lacks identifiable homologs of the MinCDE system [15]. Perhaps in the absence of the MinCDE system, ClpX-FtsZ interactions could restrict Z-ring assembly to midcell sites in M. tuberculosis.

Materials and Methods

Strains and bacterial growth conditions

E. coli strains were grown in Luria-Bertani (LB) broth or LB agar supplemented with ampicillin (Amp, 50 µg ml−1) or kanamycin (Km, 50 µg ml−1) or hygromycin (Hyg, 200 µg ml−1). M. tuberculosis strains were propagated in Middlebrook 7H9 broth supplemented with OADC (oleic acid, albumin, dextrose, catalase with sodium chloride), 0.05% tween 80 and appropriate antibiotics (Km at 25 µg ml−1; Hyg at 50 µg ml−1). When needed, strains were plated on 7H10 agar (BD biosciences) plates containing OADC and appropriate antibiotics. Growth was monitored by measuring absorbance at 600 nm and viability by determining the colony forming units on Middlebrook 7H10 agar plates without or with anhydrotetracycline. Recombinant M. smegmatis or M. tuberculosis strains with an additional copy of extrachromosomal or integrated clpX are referred to as merodiploid strains. Integrating and replicating plasmids were confirmed by bead-beating followed, respectively by PCR or restriction digestion of the recovered DNA as described [5], [6].

Molecular techniques

Oligonucleotide primers used in this study are listed in Supplementary Table S1. The clpX coding region was cloned in the sense orientation using primers ClpX-PacI and ClpX-SwaI or antisense orientation using asClpX-PacI and asClpX-SwaI under the inducible tetracycline (tet) promoter in pLR52, a replicating E. coli - Mycobacterium shuttle vector (Tables S1 and S2). As needed, cfp was cloned in-frame downstream of the clpX gene using CFP-XbaI and CFP-SwaI primers (Table S1). For some experiments, ftsZ-gfp or ftsZ-yfp fusions were cloned downstream of the tet or amidase promoter in an integrating vector (Table S2). Plasmids pUAB100 and pUAB200 (kind gift from Dr. Adries Steyn, UAB) were used for creating pMR118 and pMR119 (Table S2). For overproduction and purification of the recombinant ClpX protein, the clpX coding region was cloned in pET-19b vector (Novagen) and the recombinant His-ClpX fusion protein was purified on Ni-NTA affinity columns. A truncated ftsQ gene coding for the N-term 100 aa was also cloned in pET-19b vector using primers FtsQ-NdeI and FtsQN100-BamHI (see T1-S) and the recombinant protein was purified. All constructs were verified by sequencing. Recombinant plasmids were used to transform E. coli, M. smegmatis or M. tuberculosis as described [50]. Constructs used for Bacterial Adenylate Cyclase-based Two-Hybrid (BACTH) and Mycobacterial Protein Fragment Complementation (M-PFC) assays were produced using the primers described in supplementary Table S1. For M-PFC assay, ftsZ and clpX were cloned under the inducible tet promoter as expression from the constitutive hsp60 promoter caused growth defects in the host strain (Table S2; [50]). Recombinant M. tuberculosis and M. smegmatis strains were confirmed by PCR of genomic DNA or restriction digestion of recovered plasmid DNA as described [50].

Western blotting

Intracellular lysates of M. tuberculosis strains were prepared, the ClpX and FtsZ levels were quantitated by immunoblotting and normalized to SigA as described [26]. Cell lysates were resolved on NuPAGE polyacrylamide gels, transferred to PVDF membrane and probed with anti- FtsZ [6], anti- His or anti- B. subtilis ClpX antibodies (α-ClpXBS, kind gift from Dr. Ulf Gerth, Germany), diluted to 1[ratio]1000, 1[ratio]2000 and 1[ratio]25,000, respectively. Anti-σ70 antibodies (Neoclone Biotechnology, Madison, WI) that recognize SigA and anti- His-tag antibodies (Genscript) were used as recommended by the manufacturer [26]. Immunoblots were processed with the ECF Western blotting kit (GE life sciences, Piscataway, NJ) and scanned on a Bio-Rad Molecular Imager. For quantitative immunoblotting, known amounts of FtsZ or ClpX were quantified by volume analysis function of the QuantityOne software and standard curves were plotted. Lysates loaded on the same gel as the standards were then quantitated using the standard curve.


Wild type (WT) and recombinant M. tuberculosis strains were grown for various periods of time with shaking, harvested by centrifugation, washed in phosphate buffered saline, fixed in 4% paraformaldehyde (PAF), and stored at 4°C until further use. DAPI staining was done after washing off the PAF and incubating with 0.25 µg/ml DAPI for 15 min at RT. Excess stain was removed by centrifugation, cells were resuspended in PBS and viewed immediately. Brightfield and fluorescence imaging was done on a Nikon Eclipse 600 microscope equipped with a 100X Nikon Plan Fluor oil immersion objective with a numerical aperture of 1.4. The following filter sets were used for microscopy: GFP - standard fluorescein isothiocyanate filter set (Ex484–499, Em459–509, Chroma Technology); CFP (Ex426–446, Em460–500, Nikon); YFP (Ex490–510, Em520–550, Nikon); DAPI- DAPI filter set (Ex325–375, Em435–485, Chroma Technology). All images were acquired with a Photometrics Coolsnap ES camera and Metamorph 6.2 imaging software (Universal Imaging Corporation) and optimized with Adobe Photoshop 7.0. It is noteworthy that bright focused localization was obtained in some strains but not in others. Since all strains were grown and processed under similar conditions, we tend to favor an argument that diffuse signals in particular strains are related to the experimental context and are not an artifact of microscopy.

Purification of FtsZ and ClpX

His-tag fusion recombinant proteins FtsZ (pSAR1), FtsZG103S (pRR3) or FtsZD210G (pRR7), FtsZD374-76A (pLR12), FtsZΔC21 (pMK13) were purified under soluble conditions on Ni-NTA columns as described [28]. As needed, His-tag was removed by incubating the recombinant proteins with thrombin for 8 h at 4°C and the tag-free protein was recovered in the flow-through fractions on Ni-NTA column. The ClpX (pRD21) protein was prepared by isolation and subsequent solubilization of inclusion bodies using 8 M Urea. The resulting ClpX was then refolded by addition of the protein to a volume of refolding buffer containing 0.4 M L-arginine and 2% glycine to yield a final protein concentration of 0.5 mg/ml. The refolded ClpX was dialyzed and applied to a DEAE Sephacel column in column buffer (50 mM Tris-HCl pH 8.0, 50 mM NaCl and 10% glycerol), washed with column buffer, and eluted with the same buffer containing 1 M NaCl. Peak ClpX fractions were pooled, dialyzed and applied to a Ni-NTA column, washed, and eluted with 1X binding buffer (50 mM Sodium Phosphate pH 7.8, 500 mM NaCl, 10% Glycerol, 5 mM 2-Mercaptoethanol) containing I M Imidazole. Final preparations of ClpX protein were dialyzed against the storage buffer (25 mM HEPES-NaOH pH 7.2, 0.1 mM EDTA, 1 mM DTT, 50 mM NaCl, and 10% glycerol). This ClpX refolding protocol yielded protein concentrations in the range of 7 to 8 µM and the protein obtained was used in various experiments described in this study. Our innumerable attempts to obtain a more concentrated ClpX protein stock were, however, not successful. Size exclusion chromatography of purified ClpX on Superdex 200 10/300 GL column revealed that the majority of ClpX was hexameric (data not shown). Unless otherwise mentioned, the molar concentrations of ClpX in the various assays are based on monomer molecular weight.

FtsZ polymerization assays

Light scatter assays

FtsZ polymerization was examined by the right angle light scatter assay [27]. Briefly, various concentrations of FtsZ were incubated without or with ClpX protein (molarity based on monomer concentration) in 50 mM MES buffer pH 6.5 containing 100 mM KCl, 5 mM MgCl2 and 1 mM ATP at 30°C. Polymerization was initiated by the addition of GTP to 1 mM. The change in light scatter was monitored in FP6500 fluorimeter at 400 nM using a 1 nM slit. The data points were collected every 5 s for 15 min and plotted using Excel. Buffer controls for polymerization assays contained ClpX storage buffer lacking ClpX protein and the scatter data obtained were used for data normalization.

Sedimentation assay

Polymerization reactions containing FtsZ in a final volume of 50 µl were incubated at 30°C for 10 min and the polymerized FtsZ was collected by centrifugation at 80K for 10 min at 4°C. As needed, various concentrations of ClpX were added to the reaction. Supernatant and pellet fractions were separated on sodium dodecyl sulfate polyacrylamide (SDS-PA) gels, stained with Coomassie blue and scanned in a BioRad Molecular Imager using the QuantityOne software. Standard curve prepared with pure FtsZ protein was used for quantitating the FtsZ in the pellet fractions of the sedimentation assay. In some sedimentation assays 3′-(N-Methyl-anthraniloyl)-2′-deoxy-guanosine-5′-triphosphate, GMPCPP (Jena Biosciences, Germany), was used at a final concentration of 1 mM [30], [31]. As for light scatter assays, controls reactions contained an equivalent volume of ClpX storage buffer instead of the ClpX protein.

Protein-protein interaction assays

Pull-down assays: Experiments with pure proteins

Equimolar amounts of tag-free FtsZ and His-ClpX were mixed and incubated for 20 min, applied onto Ni-NTA resin in 1X binding buffer (50 mM Sodium Phosphate pH 7.8, 10% Glycerol, 5 mM 2-Mercaptoethanol, 150 mM NaCl, 0.1% CHAPS (3-[(3- Cholamidopropyl)dimethylammonio]-1- propanesulfonate) and 1% Nonidet P-40), washed 7X with 400 µl of 1X binding buffer containing 20 mM imidazole and eluted with 0.3 M imidazole. For assessing the strength of FtsZ-ClpX interactions, pull-down assays were performed in the presence of 0.2 or 0.5 M NaCl. Samples run on duplicate gels were probed with either α-FtsZ or α-ClpXBS antibodies as described above. We noted that the eluted FtsZ is not stoichimetric to His-ClpX, presumably due to loss during extensive washing steps.

Experiments with cell lysates

E. coli strains expressing full length His-ClpX (pRD21) together with S-tag-FtsZ (pLR66; Table S2) under the T7 promoter were induced, clear cellular lysates were prepared in 1X binding buffer and applied to Ni-NTA resin. Bound proteins were eluted and loaded on NuPAGE gels and analyzed by immunoblotting as described above.

Solid Phase assays

Four micrograms of purified ClpX or BSA was allowed to adsorb overnight onto the wells of a microtiter plate. After washing the excess unbound protein with phosphate-buffered saline containing 0.5% Tween-20 (PBST), the wells were blocked with 1% BSA in PBST for 1 hr at room temperature and incubated for 2 hrs with varying concentrations of FtsZ protein. Unbound FtsZ was removed and wells washed 5X with PBST. FtsZ bound to ClpX was detected with anti-FtsZTB antibodies by ELISA (AnaSpec). Wells with BSA served as negative controls.

Mycobacterial protein fragment complementation (M-PFC) assay

Recombinant M. smegmatis expressing ftsZ-dhfr[F1,2]/ftsZ-dhfr[F3]; clpX-dhfr [1], [2]/ftsZ-dhfr[3]; gcn4-dhfr[1], [2]/gcn4-dhfr[3]; clpX-dhfr[1], [2]/gcn4-dhfr[3]; dhfr[1], [2]/dhfr[3] or clpXΔN200-dhfr[1], [2]/ftsZ-dhfr[3] were selected on 7H11 agar plates containing Hyg and Km. Single colonies were patched on 7H11 plates with appropriate antibiotics in the presence/absence of various concentrations of Trimethoprim (Trim). Growth on Trim plates indicated interaction. Positive interactions were further confirmed by alamar blue assay [37]. Briefly, M. smegmatis strains expressing interacting proteins were cultured in 0.1 ml of 7H9 broth in 96-well, untreated, white polystyrene Nunc plates. All strains except ftsZ-dhfr [F1,2]/ftsZ-dhfr[F3] were grown with 10 ng/ml anhydrotetracycline (tet) for 3 h. Various concentrations of Trim were added for an additional 24 hrs at 37°C and finally incubated with 5 µl of alamar blue for 6 hrs. The plates were read in a Varian Cary Eclipse Fluorescence Spectrophotometer (Ex530 and Em590). M. smegmatis with gcn4-dhfr[1], [2]/gcn4-dhfr[3] served as control.

Bacterial two hybrid (BACTH) assay

BACTH system [35] kit was purchased from Euromedex and used as recommended. E. coli BTH101 recombinants with various combinations of plasmids (see Table S2) were selected on MacConkey agar supplemented with 100 µg/ml Amp and 50 µg/ml Km at 30°C for 24 to 36 h. For evaluating the strength of interaction, β-galactosidase activity was measured with cells grown in LB broth and samples were processed as recommended by the supplier. Reactions were started by the addition of 0.25 ml of 0.4% o-nitrophenol-β-galactoside (ONPG) and the tubes incubated at 28°C for 5 min or until a visible yellow color developed. Reactions were stopped by the addition of 0.5 ml of 1 M Na2CO3 and OD420 was recorded [35]. The enzymatic activity was defined as units per milliliter: 200× [(OD420 of the culture - OD420 in the control tube)/minutes of incubation] × dilution factor. The specific activity of β-galactosidase is defined as units/mg dry weight bacteria and 1 unit corresponds to 1 nmol of ONPG hydrolyzed per min at 28°C. At least 5-fold higher β-galactosidase activity than that measured for BTH101 carrying a single gene and an empty vector was considered indicative of an interaction. E. coli BTH101 transformants obtained with pKT25-zip and pUT18C-zip served as positive controls for complementation (Table S2).

RNA extraction and RT-qPCR

RNA was prepared from exponential cultures of M. tuberculosis strains grown in vitro or in macrophages essentially as described [51]. For some experiments RNA was isolated from WT M. tuberculosis exposed to 20 mg ml−1 cephalexin and 30 mg ml−1 lithium clavulanate for 24 hrs. For extraction of RNA from intracellular bacteria, macrophage monolayers were separated 3 days after infection, washed, suspended directly in RNAzol and processed as described [5], [51], [52]. Extraction of total RNA and synthesis of complementary strand DNA from mRNA specific to 16S rRNA and clpX using reverse transcription primers and iScript kit (BioRad) were as described [5], [51], [52]. Quantitative real time PCR (TaqMan chemistry) was carried out in a BioRad ICycler using the Taq DNA polymerase (NEB). The calculated threshold cycle (Ct) value for clpX was normalized to the Ct value for 16S rRNA and the fold expression was calculated using the formula: Fold change  = 2Δ(ΔCt) [51]. No RT RNA samples were included as negative controls. Expression data are average from 3 independent RNA preparations, each reverse transcribed and quantitated by real time PCR in triplicate. Real-time PCR conditions: initial activation at 95°C for 3 minutes; followed by 40 cycles of 95°C for 10 sec and 55°C for 30 seconds.

Supporting Information

Figure S1

FtsZ assembly is not affected by RecA: Light scatter assay for FtsZ polymerization in the presence or absence of RecA. Reactions containing 7.5 µM FtsZ mixed with storage buffer alone or storage buffer containing 3 µM RecA were initiated with GTP to a final concentration of 1 mM and followed for 15 minutes. Neither the rate and nor the extent of FtsZ polymerization was affected by RecA.

(0.17 MB TIF)

Figure S2

ClpX inhibition of FtsZ assembly: FtsZ polymerization was examined by the sedimentation assay. Reactions contained varying amounts of FtsZ polymerized without (A) or with a fixed concentration of ClpX at 2 µM (B). Polymerized FtsZ was collected by centrifugation and supernatant (S) and pellet (P) fractions were loaded on SDS-PA and visualized by Coomassie staining.

(0.15 MB TIF)

Figure S3

Addition of ClpX interferes to the preformed FtsZ polymers: Sedimentation assay was performed as described above with 5.4 µM FtsZ and 2 µM ClpX. For reactions 2 and 3, ClpX or storage buffer, respectively, was added at the same time as FtsZ. For reactions 4 and 5, FtsZ polymers were preformed for 5 minutes and then ClpX or storage buffer was added. Some fraction of ClpX in the pellet fractions is presumably due to its oligomerization/aggregation [20].

(0.21 MB TIF)

Figure S4

Characterization of ClpX-FtsZ interaction: (A) Strength of FtsZ-ClpX interaction. Pull-down assay using His-ClpX and tag-free FtsZ was performed in buffers containing 0.2 M and 0.5 M NaCl (see materials and methods for details). Load (L), wash (W) and elution (E) fractions were analyzed by immunoblotting. (B) FtsZ-ClpX complex isolated from cell free lysates. Cellular lysates from E. coli strain expressing his-clpXTB and ftsZTB-S-tag were loaded on NiNTA column and pull-down assay performed as described in the text. Load (L), wash (W) and elution (W) fractions were analyzed by immunoblotting as described above.

(1.41 MB TIF)

Figure S5

ClpXΔN200 does not interact with FtsZ in BACTH (A) and MPFC (B) assays. ClpXΔN200 was cloned in BACTH or MPFC vectors (Table 1) and used along with respective FtsZ constructs in the two hybrid assays as described for figures 4A and 4B.

(0.24 MB TIF)

Figure S6

ClpX expression in M.tuberculosis antisense ClpX strain. Antisense ClpX strain was propagated in Middlebrook 7H9 broth, RNA was extracted and clpX mRNA levels were determined by quantitative real time PCR. clpX mRNA levels were normalized to 16S rRNA and data are expressed with respect to levels in WT strain grown in broth. Mean ± SD from two independent experiments are shown.

(0.14 MB TIF)

Figure S7

Overproduction of ClpX does not affect intracellular FtsZ levels. FtsZ levels in M. tuberculosis clpX overexpression (A) and underexpression (B) strains were examined by quantitative immunoblotting. M. tuberculosis cellular lysates were resolved on a 10% NuPage gel, transferred to PVDF membrane and probed with α-FtsZ or α-sigma70 antibodies. FtsZ and SigA bands were quantitated using the volume analysis function of the QuantityOne Software.

(0.24 MB TIF)

Figure S8

The viability of M. tuberculosis merodiploids overproducing ClpX (ClpX) and depleted in ClpX (asClpX). Broth-grown strains were spread on the plates containing 100 ng/ml anhydrotetracycline. Grown colonies were counted and data plotted using Microsoft Excel. Mean ± SD from three independent experiments are shown.

(0.13 MB TIF)

Table S1

(0.07 MB DOC)

Table S2

(0.11 MB DOC)


We thank the members of the Madiraju and Rajagopalan labs for helpful discussions and Krishna Sarva, Maha Al Zayer, Hava Lofton and Ashwini Chauhan for technical assistance. We also thank Dr. Ulf Gerth for the kind gift of antibodies to B. subtilis ClpX and Dr. A. Steyn for the MPFC system.


Competing Interests: The authors have declared that no competing interests exist.

Funding: Funded by NIH grants RO1AI48417 (MR) and RO1AI73966, AI084734 (MM). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Gandhi NR, Moll A, Sturm AW, Pawinski R, Govender T, et al. Extensively drug-resistant tuberculosis as a cause of death in patients co-infected with tuberculosis and HIV in a rural area of South Africa. Lancet. 2006;368:1575–1580. [PubMed]
2. Smith I. Mycobacterium tuberculosis pathogenesis and molecular determinants of virulence. Clin Microbiol Rev. 2003;16:463–496. [PMC free article] [PubMed]
3. Margolin W. Themes and variations in prokaryotic cell division. FEMS Microbiol Rev. 2000;24:531–548. [PubMed]
4. Romberg L, Levin PA. Assembly dynamics of the bacterial cell division protein FTSZ: poised at the edge of stability. Annu Rev Microbiol. 2003;57:125–154. [PubMed]
5. Chauhan A, Lofton H, Maloney E, Moore J, Fol M, et al. Interference of Mycobacterium tuberculosis cell division by Rv2719c, a cell wall hydrolase. Mol Microbiol. 2006;62:132–147. [PubMed]
6. Dziadek J, Rutherford SA, Madiraju MV, Atkinson MA, Rajagopalan M. Conditional expression of Mycobacterium smegmatis ftsZ, an essential cell division gene. Microbiology. 2003;149:1593–1603. [PubMed]
7. Errington J, Daniel RA, Scheffers DJ. Cytokinesis in bacteria. Microbiol Mol Biol Rev. 2003;67:52–65, table of contents. [PMC free article] [PubMed]
8. Del Sol R, Mullins JG, Grantcharova N, Flardh K, Dyson P. Influence of CrgA on assembly of the cell division protein FtsZ during development of Streptomyces coelicolor. J Bacteriol. 2006;188:1540–1550. [PMC free article] [PubMed]
9. Frees D, Savijoki K, Varmanen P, Ingmer H. Clp ATPases and ClpP proteolytic complexes regulate vital biological processes in low GC, Gram-positive bacteria. Mol Microbiol. 2007;63:1285–1295. [PubMed]
10. Gottesman S. Proteolysis in bacterial regulatory circuits. Annu Rev Cell Dev Biol. 2003;19:565–587. [PubMed]
11. Jenal U, Fuchs T. An essential protease involved in bacterial cell-cycle control. EMBO J. 1998;17:5658–5669. [PubMed]
12. Hanson PI, Whiteheart SW. AAA+ proteins: have engine, will work. Nat Rev Mol Cell Biol. 2005;6:519–529. [PubMed]
13. Kannan N, Haste N, Taylor SS, Neuwald AF. The hallmark of AGC kinase functional divergence is its C-terminal tail, a cis-acting regulatory module. Proc Natl Acad Sci U S A. 2007;104:1272–1277. [PubMed]
14. Singh SK, Rozycki J, Ortega J, Ishikawa T, Lo J, et al. Functional domains of the ClpA and ClpX molecular chaperones identified by limited proteolysis and deletion analysis. J Biol Chem. 2001;276:29420–29429. [PubMed]
15. Cole ST, Brosch R, Parkhill J, Garnier T, Churcher C, et al. Deciphering the biology of Mycobacterium tuberculosis from the complete genome sequence. Nature. 1998;393:537–544. [PubMed]
16. Engels S, Schweitzer JE, Ludwig C, Bott M, Schaffer S. clpC and clpP1P2 gene expression in Corynebacterium glutamicum is controlled by a regulatory network involving the transcriptional regulators ClgR and HspR as well as the ECF sigma factor sigmaH. Mol Microbiol. 2004;52:285–302. [PubMed]
17. Viala J, Mazodier P. ClpP-dependent degradation of PopR allows tightly regulated expression of the clpP3 clpP4 operon in Streptomyces lividans. Mol Microbiol. 2002;44:633–643. [PubMed]
18. Chien P, Perchuk BS, Laub MT, Sauer RT, Baker TA. Direct and adaptor-mediated substrate recognition by an essential AAA+ protease. Proc Natl Acad Sci U S A. 2007;104:6590–6595. [PubMed]
19. Camberg JL, Hoskins JR, Wickner S. ClpXP protease degrades the cytoskeletal protein, FtsZ, and modulates FtsZ polymer dynamics. Proc Natl Acad Sci U S A 2009 [PubMed]
20. Sugimoto S, Yamanaka K, Nishikori S, Miyagi A, Ando T, et al. AAA+ chaperone ClpX regulates dynamics of prokaryotic cytoskeletal protein FtsZ. J Biol Chem. 2010;285:6648–6657. [PMC free article] [PubMed]
21. Farrell CM, Grossman AD, Sauer RT. Cytoplasmic degradation of ssrA-tagged proteins. Mol Microbiol. 2005;57:1750–1761. [PubMed]
22. Lu C, Stricker J, Erickson HP. FtsZ from Escherichia coli, Azotobacter vinelandii, and Thermotoga maritima—quantitation, GTP hydrolysis, and assembly. Cell Motil Cytoskeleton. 1998;40:71–86. [PubMed]
23. Flynn JM, Neher SB, Kim YI, Sauer RT, Baker TA. Proteomic discovery of cellular substrates of the ClpXP protease reveals five classes of ClpX-recognition signals. Mol Cell. 2003;11:671–683. [PubMed]
24. Haeusser DP, Lee AH, Weart RB, Levin PA. ClpX inhibits FtsZ assembly in a manner that does not require its ATP hydrolysis-dependent chaperone activity. J Bacteriol. 2009;191:1986–1991. [PMC free article] [PubMed]
25. Weart RB, Nakano S, Lane BE, Zuber P, Levin PA. The ClpX chaperone modulates assembly of the tubulin-like protein FtsZ. Mol Microbiol. 2005;57:238–249. [PubMed]
26. Chauhan A, Madiraju MV, Fol M, Lofton H, Maloney E, et al. Mycobacterium tuberculosis cells growing in macrophages are filamentous and deficient in FtsZ rings. J Bacteriol. 2006;188:1856–1865. [PMC free article] [PubMed]
27. Mukherjee A, Lutkenhaus J. Analysis of FtsZ assembly by light scattering and determination of the role of divalent metal cations. J Bacteriol. 1999;181:823–832. [PMC free article] [PubMed]
28. Rajagopalan M, Atkinson MA, Lofton H, Chauhan A, Madiraju MV. Mutations in the GTP-binding and synergy loop domains of Mycobacterium tuberculosis ftsZ compromise its function in vitro and in vivo. Biochem Biophys Res Commun. 2005;331:1171–1177. [PubMed]
29. Galletto R, Kowalczykowski SC. RecA. Curr Biol. 2007;17:R395–397. [PubMed]
30. Dajkovic A, Lan G, Sun SX, Wirtz D, Lutkenhaus J. MinC spatially controls bacterial cytokinesis by antagonizing the scaffolding function of FtsZ. Curr Biol. 2008;18:235–244. [PubMed]
31. Dajkovic A, Mukherjee A, Lutkenhaus J. Investigation of regulation of FtsZ assembly by SulA and development of a model for FtsZ polymerization. J Bacteriol. 2008;190:2513–2526. [PMC free article] [PubMed]
32. White EL, Ross LJ, Reynolds RC, Seitz LE, Moore GD, et al. Slow polymerization of Mycobacterium tuberculosis FtsZ. J Bacteriol. 2000;182:4028–4034. [PMC free article] [PubMed]
33. Hett EC, Chao MC, Deng LL, Rubin EJ. A mycobacterial enzyme essential for cell division synergizes with resuscitation-promoting factor. PLoS Pathog. 2008;4:e1000001. [PMC free article] [PubMed]
34. Rajagopalan M, Maloney E, Dziadek J, Poplawska M, Lofton H, et al. Genetic evidence that mycobacterial FtsZ and FtsW proteins interact, and colocalize to the division site in Mycobacterium smegmatis. FEMS Microbiol Lett. 2005;250:9–17. [PubMed]
35. Karimova G, Dautin N, Ladant D. Interaction network among Escherichia coli membrane proteins involved in cell division as revealed by bacterial two-hybrid analysis. J Bacteriol. 2005;187:2233–2243. [PMC free article] [PubMed]
36. Datta P, Dasgupta A, Singh AK, Mukherjee P, Kundu M, et al. Interaction between FtsW and penicillin-binding protein 3 (PBP3) directs PBP3 to mid-cell, controls cell septation and mediates the formation of a trimeric complex involving FtsZ, FtsW and PBP3 in mycobacteria. Mol Microbiol. 2006;62:1655–1673. [PubMed]
37. Singh A, Mai D, Kumar A, Steyn AJ. Dissecting virulence pathways of Mycobacterium tuberculosis through protein-protein association. Proc Natl Acad Sci U S A. 2006;103:11346–11351. [PubMed]
38. Datta P, Dasgupta A, Bhakta S, Basu J. Interaction between FtsZ and FtsW of Mycobacterium tuberculosis. J Biol Chem. 2002;277:24983–24987. [PubMed]
39. Ma X, Margolin W. Genetic and functional analyses of the conserved C-terminal core domain of Escherichia coli FtsZ. J Bacteriol. 1999;181:7531–7544. [PMC free article] [PubMed]
40. Mosyak L, Zhang Y, Glasfeld E, Haney S, Stahl M, et al. The bacterial cell-division protein ZipA and its interaction with an FtsZ fragment revealed by X-ray crystallography. EMBO J. 2000;19:3179–3191. [PubMed]
41. Corbin BD, Wang Y, Beuria TK, Margolin W. Interaction between cell division proteins FtsE and FtsZ. J Bacteriol. 2007;189:3026–3035. [PMC free article] [PubMed]
42. Sassetti CM, Boyd DH, Rubin EJ. Genes required for mycobacterial growth defined by high density mutagenesis. Mol Microbiol. 2003;48:77–84. [PubMed]
43. Sureka K, Hossain T, Mukherjee P, Chatterjee P, Datta P, et al. Novel role of phosphorylation-dependent interaction between FtsZ and FipA in mycobacterial cell division. PLoS One. 2010;5:e8590. [PMC free article] [PubMed]
44. Goley ED, Iniesta AA, Shapiro L. Cell cycle regulation in Caulobacter: location, location, location. J Cell Sci. 2007;120:3501–3507. [PubMed]
45. Kelly AJ, Sackett MJ, Din N, Quardokus E, Brun YV. Cell cycle-dependent transcriptional and proteolytic regulation of FtsZ in Caulobacter. Genes Dev. 1998;12:880–893. [PubMed]
46. Gerth U, Kirstein J, Mostertz J, Waldminghaus T, Miethke M, et al. Fine-tuning in regulation of Clp protein content in Bacillus subtilis. J Bacteriol. 2004;186:179–191. [PMC free article] [PubMed]
47. Chen Y, Anderson DE, Rajagopalan M, Erickson HP. Assembly dynamics of Mycobacterium tuberculosis FtsZ. J Biol Chem. 2007;282:27736–27743. [PMC free article] [PubMed]
48. Anderson DE, Gueiros-Filho FJ, Erickson HP. Assembly dynamics of FtsZ rings in Bacillus subtilis and Escherichia coli and effects of FtsZ-regulating proteins. J Bacteriol. 2004;186:5775–5781. [PMC free article] [PubMed]
49. Stricker J, Maddox P, Salmon ED, Erickson HP. Rapid assembly dynamics of the Escherichia coli FtsZ-ring demonstrated by fluorescence recovery after photobleaching. Proc Natl Acad Sci U S A. 2002;99:3171–3175. [PubMed]
50. Dziadek J, Madiraju MV, Rutherford SA, Atkinson MA, Rajagopalan M. Physiological consequences associated with overproduction of Mycobacterium tuberculosis FtsZ in mycobacterial hosts. Microbiology. 2002;148:961–971. [PubMed]
51. Fol M, Chauhan A, Nair NK, Maloney E, Moomey M, et al. Modulation of Mycobacterium tuberculosis proliferation by MtrA, an essential two-component response regulator. Mol Microbiol. 2006;60:643–657. [PubMed]
52. Nair N, Dziedzic R, Greendyke R, Muniruzzaman S, Rajagopalan M, et al. Synchronous replication initiation in novel Mycobacterium tuberculosis dnaA cold-sensitive mutants. Mol Microbiol. 2009;71:291–304. [PMC free article] [PubMed]

Articles from PLoS ONE are provided here courtesy of Public Library of Science