- Research article
- Open Access
Inositol monophosphate phosphatase genes of Mycobacterium tuberculosis
© Movahedzadeh et al; licensee BioMed Central Ltd. 2010
Received: 8 April 2009
Accepted: 18 February 2010
Published: 18 February 2010
Mycobacteria use inositol in phosphatidylinositol, for anchoring lipoarabinomannan (LAM), lipomannan (LM) and phosphatidylinosotol mannosides (PIMs) in the cell envelope, and for the production of mycothiol, which maintains the redox balance of the cell. Inositol is synthesized by conversion of glucose-6-phosphate to inositol-1-phosphate, followed by dephosphorylation by inositol monophosphate phosphatases (IMPases) to form myo-inositol. To gain insight into how Mycobacterium tuberculosis synthesises inositol we carried out genetic analysis of the four IMPase homologues that are present in the Mycobacterium tuberculosis genome.
Mutants lacking either impA (Rv1604) or suhB (Rv2701c) were isolated in the absence of exogenous inositol, and no differences in levels of PIMs, LM, LAM or mycothiol were observed. Mutagenesis of cysQ (Rv2131c) was initially unsuccessful, but was possible when a porin-like gene of Mycobacterium smegmatis was expressed, and also by gene switching in the merodiploid strain. In contrast, we could only obtain mutations in impC (Rv3137) when a second functional copy was provided in trans, even when exogenous inositol was provided. Experiments to obtain a mutant in the presence of a second copy of impC containing an active-site mutation, in the presence of porin-like gene of M. smegmatis, or in the absence of inositol 1-phosphate synthase activity, were also unsuccessful. We showed that all four genes are expressed, although at different levels, and levels of inositol phosphatase activity did not fall significantly in any of the mutants obtained.
We have shown that neither impA, suhB nor cysQ is solely responsible for inositol synthesis. In contrast, we show that impC is essential for mycobacterial growth under the conditions we used, and suggest it may be required in the early stages of mycothiol synthesis.
Mycobacterium tuberculosis is a major global pathogen. In 2007, approximately 1.7 million deaths were caused by tuberculosis (TB) and an estimated 9.3 million people acquired the infection . Patients can usually be cured through a six month course of a multiple drug regimen . The efficacy of chemotherapy has however been compromised by the appearance of multi- and extensively drug resistant strains [3, 4]. The search for potential novel drug targets and the subsequent development of new antibiotics is therefore urgent. Ideal candidates would be mycobacterial-specific and include pathways involved in the biosynthesis of the unusual cell envelope [5, 6]; the target of some existing antibiotics, including isoniazid, ethionamide, ethambutol and pyrazinamide .
Inositol is a polyol that is not synthesized in most bacterial species. However, in the mycobacteria, inositol is found in lipoarabinomannan (LAM), a lipoglycan that is present in high levels in the cell envelope. LAM is composed of a mannan backbone with branched arabinosyl chains. It is anchored in the cell envelope by means of a phosphatidylinositol (PI) moiety. Other lipoglycans found in the cell envelope include lipomannan (LM) and PI mannosides (PIMs). PI-containing molecules have been demonstrated as essential for growth in the fast-growing species Mycobacterium smegmatis, as mutants lacking PI synthase are not viable .
The function of LAM in cell envelope integrity is unknown, but evidence suggests that it has profound effects on the host., for example, it stimulates macrophages to produce TNFα , nitric oxide , and matrix metalloproteinases . LAM may therefore play a major role in the stimulation of an inappropriate host immune response, leading to the pathology that is characteristic of TB. LAM also induces transcriptional activation of HIV-1 [12, 13] and may play a role in the synergy seen between HIV and TB. In addition to these effects, LAM is a major antigen [14, 15]. While some PIMs are probable precursors of LAM, they may also have important functions of their own. PI dimannoside (PIM2), for example, has been implicated as a receptor for interacting with mammalian cells , as a secreted activator of Toll-like receptor 2 in macrophages leading to TNFα induction , and as an inducer of granuloma formation .
Inositol is also a constituent of the major mycobacterial thiol, mycothiol (1-D-myo-inosityl-2- [N-acetyl-L-cysteinyl] amido-2-deoxy-α-D-glucopyranoside) [19, 20], which helps maintain the redox state of the cell and detoxifies harmful molecules. A mutant of M. smegmatis that essentially fails to produce mycothiol is viable, but grows poorly, and is sensitive to H2O2  However, in M. tuberculosis the mshA and mshC genes, required for mycothiol biosynthesis, are essential genes [21, 22]. Mycothiol may be more important in pathogenic mycobacteria as during infection they would be exposed to reactive oxygen intermediates within the macrophage.
The biosynthesis of inositol normally occurs in two steps. In the first, glucose-6-phospate is converted to inositol-1-phosphate (I-1-P) by inositol phosphate synthase (Ino1). We have shown previously that an ino1 (Rv0046c) mutant of M. tuberculosis is an inositol auxotroph, and is severely attenuated in vivo . In the second step, the I-1-P is dephosphorylated by an inositol monophosphate phosphatase (IMPase) to form inositol. Previously, we identified the M. smegmatis impA gene, which is predicted to encode an IMPase, and showed that inactivation of this gene resulted in an altered colony morphology, reduced levels of PI dimannoside (PIM2), and altered permeability of the cell wall. This data suggests that impA is partly responsible for inositol synthesis in this species, presumably compensated by the presence of other imp genes . In this paper, we describe the genetic analysis of four IMPase homologues of M. tuberculosis. We demonstrate that three, impA, suhB and cysQ are dispensible, while impC is essential, even in the presence of exogenous inositol.
Bacterial strains, plasmids and media
M. tuberculosis strains and plasmids
E. coli DH5α
M. tuberculosis H37Rv
wild-type laboratory strain
M. tuberculosis suhBΔ
M. tuberculosis impAΔ
M. tuberculosis impCΔ::pFM96
M. tuberculosis::pFM54 (impCΔ SCO)
M. tuberculosis ino1Δ
M. tuberculosis ino1Δ::pFM54 (SCO)
M. tuberculosis::pFM151 (cysQΔ SCO)
pBluescript II SK+
pUC-based plasmid with Hin dIII cassette carrying gm and L5 int
pUC-based plasmid with Hin dIII cassette carrying hyg and L5 int
gene manipulation vector, kan
hyg pAg85-lacZ sacB Pac I cassette vector
pGEM5::impAΔ (Sph I 200 bp)
p2NIL::impAΔ (Sph I 200 bp)
p2NIL::impAΔ (769 bp)
pFM74 with Pac I cassette of pGOAL19
pFM48 with Pac I cassette of pGOAL19
pFM53 with Pac I cassette of pGOAL19
pBluescript SK+::impC (+288 bp upstream)
plasmid carrying the M. smegmatis porin gene mspA
pFM148 with Pac I cassette of pGOAL19
pBluescript SK+::cysQ (+352 bp upstream)
Homology searches were carried out using BLASTP ver 2.2.13  The four homologs identified all had e-values <10-3, and no other protein match approached significance. Prosite database information was obtained at http://www.expasy.ch/prosite/, using Release 20.56 dated November 4th, 2009.
Construction of M. tuberculosis mutants
Targeted mutagenesis was carried out using a two-step strategy  in order to introduce an unmarked mutation without any potential polar effects.
Primers tbimpA1 (CTCGACGTACAGGTTGAGCTATCC) and tbimpA2 (CTTCACCTGACCGATCGTCAGCTC) were used to amplify the impA gene and flanking regions (2,108 bp) from M. tuberculosis H37Rv using PCR. The resulting 2.1 kb fragment was cloned into the Eco RV site of pGEM5, producing pIMP50. A 200 bp Sph I fragment within impA was removed following partial digestion and religated to make pIMP51. The 2,348 bp Pvu II fragment of pIMP51 was cloned into p2NIL, producing pIMP57.
To create a deletion where the majority of impA was deleted (769 bp deleted from 813 bp), inverse PCR was performed on pIMP57. Primers tbimpAinv1 (TCGTGCCAGCTGACCAACGAATCCAAGTGCAT) and tbimpAinv2 (TCGTGCCAGCTGATAGGGGAACCAGAGGACTA) were used, simultaneously creating a deletion and introducing a Pvu II site in the deleted construct. Following the PCR reaction the DNA was digested with Dpn I for 1 h at 37C to destroy the template, then digested with Pvu II and religated to produce pFM74. Insertion of a Pac I gene cassette from pGOAL19 was cloned at the Pac I site of pFM74 producing the final delivery plasmid pFM75. The Pac I cassette carries lacZ and sacB, which can be used for positive and negative selection of unmarked mutant colonies, respectively.
A 3,534 bp Xho I fragment of cosmid Y5ab was cloned into the Sal I site of plasmid p2NIL to produce pFM33. A fragment of 817 bp was deleted from the 874 suhB gene by inverse PCR on pFM33 using primers tbsuhBΔ1 (TCAGCATGCGTTCGTTGTCAGGTCGTGTC) & tbsuhBΔ2 (TCAGCATGCGATTCAACGGCCTAGAGC); this introduced a Sph I site in the deleted construct. Following treatment with Dpn I and Sph I, this was religated to produce pFM48. Insertion of the gene delivery cassette from pGOAL19 produced the final delivery plasmid pFM52.
A 2,503 bp Stu I fragment of cosmid Y3A2 was cloned into the Pml I site of p2NIL, producing pFM31. A 731 bp deletion was generated in the 783 bp gene by inverse PCR on pFM31 using primers tbimpCΔ1 (TGCCAGCTGCATTAGATCGTCGTGGCTCA) & tbimpCΔ2 (TGCCAGCTGGAGGTGCTGACACGGCTC) to introduce a Pvu II site in the deleted construct. Following treatment with Dpn I and Pvu II, this was religated to produce pFM53. Insertion of the delivery gene cassette from pGOAL19 produced the final delivery plasmid pFM54.
Primers tbcysQ1 (CCTGGTCGACCTGTTTCC) and tbcysQ2 (GCGGCTCTTTGACATCTTGT) were used to amplify the cysQ gene and flanking regions (2,748 bp) from M. tuberculosis H37Rv DNA. The product was cloned into the Pml I site of p2NIL, producing pFM145. Primers tbcysQΔ1 (AGTCAGGTCGTCCGTCAGATC) & tbcysQΔ2 (TACAACCAACTGGACCCCTAC) were used to generate a 666 bp deletion in the 804 cysQ gene by inverse PCR on pFM145. Following treatment with Klenow polymerase and T4 polynucleotide kinase (Promega), this product was religated to produce pFM148. Insertion of the gene delivery cassette from pGOAL19 produced the final delivery plasmid pFM151.
Deletion plasmids were constructed as described above. The delivery plasmids were introduced into M. tuberculosis H37Rv or M. tuberculosis H37Rv ino1, and single crossovers (SCOs) isolated by selection for blue hygR kanR colonies. One SCO colony was plated onto 2% (wt/vol) sucrose-50 μg ml-1 X-Gal to isolate bacteria with a second crossover; this will lead to mutant or wild-type cells depending on the location of the recombination event. In order to screen for impC mutant, DNA was extracted from sucroseS kanS white colonies (obtained from plating M. tuberculosis FAME9 onto sucrose medium) and analysed by PCR using primers that flank the impC gene (TBC1: GGACCGCGATCAGTATGAGT and TBC2: TCGACACAGAATCCGCTAGA). Strains carrying the impC wild-type allele would produce a band of 1148 bp whereas strains carrying an impC mutation would carry the deletion band of 417 bp. Mutant candidates and a wild-type control were digested with Pvu II and subjected to Southern blot analysis using a 2.5 kb impC probe (impC plus flanking region). The wild-type strain showed a 4 kb band whilst the mutant showed a 3.2 kb deletion band along with a 2.5 kb band for the integrated impC copy
A construct expressing the impC gene was made by PCR amplification of the impC gene, together with 288 bp of upstream sequence using chromosomal M. tuberculosis H37Rv as template DNA. The primers tbimpCBamP (CGCGGATCCGGCGATGGTGACAT) and tbimpCBam (CGCGGATCCTTACCCGGCGTTGAGC) were used. The product was digested with Bam HI and cloned into the Bam HI site of pBluescript-SK+ to produce pFM94. The Hin dIII cassette of pUC-Gm-int, carrying the int and gm genes was cloned into the Hin dIII site of pFM94 to produce pFM96.
A construct expressing the cysQ gene was made by PCR amplification of the cysQ gene including 352 bp of upstream sequence using M. tuberculosis H37Rv; chromosomal template DNA; primers tbcysup (GCATAGAGCAGGAGGTTTGC) and tbcysend (GCGCCACGCGTCGGCGAT) were used. The PCR product was treated with T4 polynucleotide kinase and cloned into the Sma I site of pBluescript-SK+ to produce pFM160. The Hin dIII cassette of pUC-Gm-int, carrying the int and gm genes was cloned into the Hin dIII site of pFM160 to produce pFM164.
Site-directed mutagenesis was carried out using the non-PCR-based Quickchange kit (Stratagene). Oligonucleotides D86N-forward (GGATCGTAGACCCGATCAACGGCACCAAAAACTTTGTGC) & D86N-reverse (GCACAAAGTTTTTGGTGCCGTTGATCGGGTCTACGATCC) were used to prime DNA synthesis with pFM96. Sequencing confirmed the presence of the required mutation.
Real-time quantitative PCR
Primers used in Real time quantitative PCR
Cell wall analysis
Extraction and analysis of PIMs
Cells (0.2 g) were delipidated with chloroform/methanol (1/1, v/v) for 48 h at room temperature with continuous stirring. Lipids were separated from the delipidated cells by centrifugation (3000 rpm, 15 min, 2600 xg) and analysed by TLC on silica gel-coated plates developed with chloroform/methanol/water (60:35:8, v/v/v). The various PIMs were identified by their mobilities on TLC and their positive reactivity compared to authentic standards; these included a sugar and phospholipid-specific reagent (0.2% anthrone in concentrated H2SO4 followed by heating) and the Dittmer-Lester reagent that specifically detects phosphorous-containing lipids, respectively .
Production and analysis of LAM and LM
Delipidated cells were washed and disrupted using a Cell disrupter (2 kbars, Constant System Ltd; one shot model). The resulting material was extracted with 40 mL ethanol/water (1/1, v/v) for 8 h at 65°C; the bacterial residues were discarded and the supernatant was dried. Six ml hot phenol/water (1/1, v/v) were added and the mixture was heated for 1 h at 70°C under continuous stirring, followed by a two-phase partition. The phenol phase was discarded and the upper phase extensively washed and dried. The extract was solubilised in water and Triton X114 (2% wt/v) was added to the cooled suspension. The mixture was stirred for 10 min and then heated at 50°C until two phases formed. The detergent phase was recovered, diluted by adding 1 ml water and washed three times with CHCl3. The resulting aqueous phase was dried to evaporate the chloroform and resuspended in water (0.2 ml). This portion was analysed by SDS-PAGE with a 5% stacking gel and a 15% running gel. Samples were denatured in the presence of 2% SDS in 50 mM Tris-HCl (pH 6.8). After electrophoresis, gels were treated with periodate/ethanol/acetic acid (0.7/40/5, w/v/v), and silver-stained. Authentic samples of mycobacterial LAM and LM from Mycobacterium bovis BCG were used as standard.
Sugar compositional analysis
The sugar constituents of the various materials were determined after acid hydrolysis with 2 M CF3COOH at 110°C for 1 h; the mixture of hydrolysed products was dried, treated with trimethylsilyl reagents  to derivatise monosaccharides and analysed by gas chromatography (GC) for their sugars.
Gas chromatography and mass spectrometry
GC was performed using a Hewlett Packard HP4890A equipped with a fused silica capillary column (25 m length × 0.22 mm i.d.) containing WCOT OV-1 (0.3 mm film thickness, Spiral). A temperature gradient of 100-290°C at 5°C min-1, followed by a 10-min isotherm plateau at 290°C, was used.
Labelling of cell extracts with monobromobimane (mBBr) to determine thiol content was performed with modifications to previously published protocols [31, 32]. Cell pellets from 3 ml culture were resuspended in 0.5 ml of warm 50% acetonitrile-water containing 2 mM mBBr (Cal Biochem), and 20 mM HEPES-HCl, pH 8.0. The suspension was incubated for 15 min in a 60°C water bath and then cooled on ice. A final acidic pH was produced by adding 2-5 μl 5 M HCl or 5 M trifluoracetic acid.
The control samples were extracted with 0.5 ml of warm 50% acetonitrile-water containing 5 mM N-ethylmalemide and 20 mM HEPES-HCl, pH 8.0. The suspension was incubated for 15 min in a 60°C water bath and then cooled on ice. 2 mM mBBR were added to the solution followed by a second incubation for 15 min in a 60°C. The control sample was cooled but not acidified. Cell debris was pelleted in each sample by centrifugation (5 min 14,000 × g).
HPLC analysis of thiols was carried out by injecting 25 μl of 1:4 dilution of samples in 10 mM HCl on to a Beckman Ultrasphere IP 5 μ(250 mm × 4.6 mm) column using 0.25% glacial acetic acid pH 3.6 (buffer A) and 95% methanol (buffer B). The gradient was: 0 min, 10% B; 15 min, 18% B; 30 min, 27% B; 32 min, 100% B; 34 min, 10% B; and 60 min, 10% B (reinjection). The flow rate was 1 ml min-1, and the fluorescence detection was accomplished on a Varian Fluorichrom model 430020 with a 370 nm excitation filter and a 418-700 nm emission filter. Data collection and analysis was performed on Dynamax Mac Integrator (Rainin Instruments).
Bacteria were grown to mid-log phase, and collected by centrifugation. Each pellet was washed once in distilled water followed by resuspension in 2.5 ml 2 mM dithiothreitol in 50 mM Tris-Cl, pH8. The suspended bacteria were disrupted in a FastPrep220A at 4 m/sec for 3 cycles of 20 sec in Lysing Matrix B (0.1 mm silica beads), with cooling on ice between cycles. The resulting cell-extracts were then clarified at 4000 g for 4 min using a bench centrifuge and filter-sterilised through 0.2 μm pore cellulose acetate filters (Sartorius Minisart). Each clarified cell extract was desalted through Pharmacia PD-10 columns according to the manufacturer's instructions; with the exception that 3.2 ml (not 3.5 ml) protein fraction was collected. For equilibrating, desalting and eluting using PD-10, 50 mM Tris-Cl, pH8 was used.
Phosphatase assays were conducted using 0.4 mM substrates at 37°C, as described previously  although the reaction volume used was 120 μl and was stopped with 30 μl malachite green reagent. No precipitates were formed so the entire assay was performed in ELISA plate wells. Inorganic phosphate present in each well was calculated by reading the OD against a standard curve. Enzyme activity was then calculated by subtracting the phosphate formed in wells with cell extract and substrate, from phosphate formed in corresponding wells with cell extract but without substrate.
These four genes are generally conserved in other actinomycete genomes, with for example, apparent orthologs in Mycobacterium avium, Mycobacterium smegmatis, and Corynebacterium glutamicum (data not shown). M. leprae, which has many pseudogenes, has no functional impA. Other genomes do also have a small number of other IMPase genes (thus, M. avium has a fifth paralog that is similar to cysQ). While levels of homology between the different M. tuberculosis IMPase paralogs are moderate (22-30% amino acid identity), similarities between orthologs are much higher (for example, 75-79% identity between M. tuberculosis and M. leprae, and 51-67% identity between M. tuberculosis and M. smegmatis).
The suhB gene (Rv2701c) was named in the original genome annotation , because it is the gene most similar to the Escherichia coli suhB gene. The E. coli suhB gene was so-named because deletion of the gene resulted in a cold-sensitive phenotype, and suppression of a thermosensitive rpoH mutation . It has also been shown to suppress secY , dnaB , and era  mutations. However, these phenotypes are not related to the enzymatic properties of the protein, as they are unaffected by a null point mutation in the active site  (Figure 1B). Furthermore, inositol production is not believed to occur in E. coli, so the biological context is very different from that in mycobacteria. Recombinant SuhB from M. tuberculosis has been confirmed to have IMPase activity . SuhB is monocistronic in M. tuberculosis (Figure 2).
The third homologous gene is Rv3137, which we have called impC. It appears to be the first gene in a two-gene operon; a 457 bp intergenic gap upstream of impC suggests it has its own promoter., and a second gene, pflA, is predicted to start only 14 bp downstream, so is probably co-transcribed. PflA shows homology to pyruvate formate lyase-activating proteins. Beyond this is a cluster of fad genes (fadE24-fadE23-fadB4), but the gap beyond pflA and fadE24 is 79 bp, so is less likely to be part of the same operon.
The fourth homologous gene is cysQ (Rv2131c), so-named because it is most similar to the E. coli cysQ gene. E. coli cysQ mutants are cysteine auxotrophs during aerobic growth . Interestingly M. smegmatis contains two paralogs of this gene.
Two sequence motifs have been described for IMPases in the Prosite database  (see legend to Figure 1B). One motif, near the N-terminus contains the metal-binding aspartate residues of the active site, and the other lies near the C-terminus. All of the gene products except SuhB had small differences from at least one of the two IMPase motifs (Figure 1B). However, they all contain the important metal-binding residues in both motifs.
The M. tuberculosis impA and suhB genes are dispensable
The impA gene has previously been shown to play an indirect role in inositol synthesis in M. smegmatis , and a knockout plasmid construct was therefore prepared to isolate an M. tuberculosis impA mutant. As the gene lies within the his operon (Figure 2), this plasmid carried an unmarked deletion that would not have polar effects. The mutant was generated using a two-step method , and grew well on solid medium. Unlike the M. smegmatis impA mutant which had altered colony morphology, there were no obvious differences in colony morphology between the wild-type and mutant strains.
We carried out a similar experiment to determine whether suhB plays a role in inositol metabolism. Again, a deletion construct was prepared, and an unmarked mutant isolated, with no obvious differences in colony morphology.
Inactivation of CysQ
We constructed a plasmid to delete the cysQ gene. Initially, we were unable to obtain a mutant; of 97 double crossovers (DCOs) screened in the presence of inositol, all were wild-type. We therefore made a merodiploid strain by integrating a second copy of cysQ into the single crossover (SCO) strain, and repeating the selection for DCOs on sucrose. Using this method, 24 out of 30 colonies were found to be mutants. The ability to isolate a mutant only in the presence of a functional copy of the gene indicates that this gene was essential under the conditions tested. It could be inferred that cysQ synthesizes all the inositol in the cell, or all the inositol for a specific essential molecule. However, this hypothesis is improbable, as, if true, we would predict thatmutants would be inositol auxotrophs, yet no mutants were isolated even in the presence of high levels of inositol. One possibility is that inositol does not penetrate the cell wall, which is known to be highly impermeable. However, as we had successfully isolated a mutant lacking inositol-1-phosphate synthase (an inositol auxotroph), only when the media was supplemented with extremely high levels of exogenous inositol (50-77 mM) , it seems that inositol does enter the cell in sufficient quantities but permeability to this molecule is poor. This suggests that even a slight increase in the requirement for inositol might make mutant isolation impossible, since we had reached the limits of inositol solubility. We reasoned that an increase in the availability of inositol by introduction of a porin might allow a mutant to be isolated. We therefore electroporated an integrating plasmid (pMN013) carrying the M. smegmatis porin gene mspA [44, 45] (for which M. tuberculosis has no orthologue) into the SCO strains, and repeated the sucrose selection. Using this method, we successfully isolated a cysQ mutant in the presence of 77 mM inositol. We screened 16 DCO colonies and two were mutants.
We then plated the mutant on inositol-free medium, and were surprised to observe normal growth, indicating that once the mutant has been isolated, it does not require inositol. To determine whether the mutant could survive in the absence of the mspA gene, the integrating plasmid containing this gene was switched with an empty integrative plasmid carrying the hygromycin resistance gene (pUC-Hyg-int). This would result in the replacement of the cysQ-carrying plasmid, leaving a stain with no functional cysQ. Surprisingly, we were able to obtain cysQ mutants using this approach although we had failed to isolate a mutant by our standard mutagenesis procedure. We therefore conclude that cysQ is also dispensible, and a cysQ mutant does not require inositol for growth.
The impC gene is essential
We attempted to construct an unmarked impC deletion mutant. The first step of the mutagenesis to produce SCOs worked well, however, when cells carrying a second crossover were isolated, only wild-type bacteria were obtained. In theory, the second crossover could take place on either side of the deletion, resulting in either mutant or wild-type cells. The fact that we obtained only wild-type cells (n = 48) suggested that the mutants are not viable.
These initial mutagenesis experiments were carried out in the absence of exogenous inositol. We therefore repeated the mutagenesis, including different levels of inositol in the media at all times. Again, only wild-type bacteria were isolated following the second cross-over (n= 97; 16 on 15 mM inositol, 8 on 30 mM, 16 on 46 mMl, and 57 on 77 mM).
The inability to obtain a mutant may be due to other factors, such as a low frequency of recombination on one side of the gene, even though the length of flanking DNA should be sufficient (847 and 874 bp). Therefore we constructed a merodiploid strain by inserting a second functional copy of impC into the SCO strain. This extra copy was present on an L5-based integrating vector, and contained 288 bp upstream of impC, which was likely to carry its promoter. When this strain (FAME9) was plated onto sucrose to isolate DCOs, three out of eight colonies isolated had lost the original copy of impC. The fact that this gene could only be lost when a second copy of the gene is present suggests that impC is essential for survival, even in the presence of high levels of exogenous inositol (Fisher's exact test, p < 0.01, comparing only the experiments with 77 mM inositol and the complemented strain). To further investigate the essentiality of the impC gene, and in view of what was observed with cysQ, we introduced the mspA gene into the impC SCO strain; this time we were not successful in obtaining a mutant, indicating that the difficulty we encountered making an impC mutant differed from cysQ.
A difference between an IMPase mutant and an ino1 mutant may be that inositol-1-phosphate accumulates in the IMPase mutant, which might somehow be detrimental to the cell. We therefore carried out the essentiality experiment in an ino1 mutant background. The impC mutant construct was introduced into M. tuberculosis ino1, and a SCO strain isolated. On plating for DCOs, only wild-type colonies were isolated (n = 38), again suggesting that this was not the explanation for the essentiality.
Site directed mutagenesis of impC
Our results suggest that impC does not have a critical role in inositol production and hence our inability to obtain an impC mutant may indicate that impC has a different or secondary function that prevents isolation of a mutant. For example, the enzyme might form part of an enzyme complex, and play a vital structural role in maintaining the integrity of that complex. Deletion of the gene would then have both enzymatic and structural effects. An analogous situation was found with the E. coli SuhB protein; where phenotypes in suhB mutants were not related to IMPase activity, as a point mutation in the active site did not produce the suppressing phenotype . We therefore used the same approach to try to separate enzymatic activity from a structural role.
A D93N change in E. coli SuhB and an equivalent D90N change in the human IMPase suppress activity [40, 46] (Figure 1B). Site-directed mutagenesis was used to introduce a corresponding mutation (D86N) in the M. tuberculosis impC gene using the integrating plasmid pFM96 previously used for complementation. This plasmid (pFM123) was introduced into the SCO strain FAME7, and the resultant strain (FAME11) was streaked onto sucrose/inositol plates. DCO colonies were analysed, and, in contrast to the situation with pFM96, all were shown to be wild-type (n = 52). The fact that the functional impC gene could not be replaced by this mutated gene, even in the presence of inositol (p < 0.01), shows that the mutation did inactivate enzymatic activity, and (assuming that the structure was not affected) that it is this enzymatic activity that is essential, rather than an additional structural role.
Phosphatases in cell extracts of impA, suhB mutants
26.04 ± 1.85 (5)
28.18 ± 0.92 (5)
32.70 ± 0.44 (5)
0.63 ± 0.13 (6)
0.79 ± 0.12 (5)
0.63 ± 0.25 (6)
1.20 ± 0.15 (4)
1.33 ± 0.22 (5)
1.03 ± 0.15 (6)
0.08 ± 0.06 (12)
-0.02 ± 0.03 (2)
0.39 ± 0.03 (2)
-0.13 ± 0.12 (12)
-0.08 ± 0.03 (2)
0 ± 0.21 (2)
4.22 ± 0.36 (8)
4.13 ± 0.40 (2)
5.74 ± 0.04 (2)
3.00 ± 0.35 (12)
3.55 ± 0.14 (2)
4.38 ± 0.36 (2)
Phosphatases in cell extracts of the cysQ mutants
18.94 ± 1.00 (6)
13.09 ± 1.24 (6)
12.41 ± 0.54 (7)
0.40 ± 0.09 (8)
0.49 ± 0.17 (9)
0.57 ± 0.16 (9)
0.84 ± 0.12 (8)
0.90 ± 0.27 (10)
0.70 ± 0.23 (10)
0.75 ± 0.32 (8)
1.02 ± 0.27 (10)
0.55 ± 0.15 (10)
-0.37 ± 0.28 (3)
-0.35 ± 0.14 (3)
0.27 ± 0.45 (3)
1.42 ± 0.31 (3)
1.69 ± 0.14 (3)
1.39 ± 0.03 (3)
5.51 ± 0.36 (2)
3.64 ± 1.92 (2)
2.83 ± 0.25 (3)
PIM, LAM and mycothiol levels are normal in the impA, suhB and cysQ mutants
Gene expression levels of imp genes in M. tuberculosis
mRNA level normalised to sigA*
0.41 (0.3- 0.5)
0.11 (0.096- 0.13)
0.36 (0.27- 0.46)
0.95 (0.76- 1.18)
To investigate how M. tuberculosis synthesises inositol, we carried out a genetic analysis of four IMPase homologues in M. tuberculosis. The impA and suhB genes were shown to be dispensable, with no phenotype detected in terms of the levels of mycothiol, PIMs, LM or LAM. CysQ is also dispensible, although isolating the mutant proved more difficult, requiring introduction of the M. smegmatis mspA porin gene for mutant isolation, but not for subsequent survival. It cannot be excluded, however, that the cysQ mutants that were eventually obtained had acquired a suppressor mutation, which had allowed deletion of cysQ or had allowed growth of the mutant on media lacking inositol and preventing cell death. In contrast to these three genes, we were only able to inactivate impC by introducing a second copy of the gene. The TraSH mutagenesis protocol which provides a genome-wide indication of essentiality  supports our data, with only impC of these four genes being reported as putatively required for optimal growth in vitro.
Inositol production is likely to be essential for mycobacterial growth, because of the essentiality of both classes of mycobacterial inositol-containing molecules, namely phospholipids  and mycothiol Our previous work showing that a PI synthase mutant is an inositol auxotroph  is consistent with this. Both SuhB and CysQ have been shown to have IMPase activity [41, 48] and we have shown that the M. smegmatis ImpA has IMPase activity (unpublished data). However, none of the three mutants constructed are auxotrophic for inositol, indicating that there is potential redundancy of function between the homologs and deletion of three or four genes might be required to see sufficient loss of activity to cause auxotrophy. A recent report suggests that CysQ is likely to play a role in sulphur metabolism, as its activity as 3'-phosphoadenosine-5'-phosphatase is several orders of magnitude higher than as an inositol phosphatase . However, it may still contribute to the redundancy in inositol phosphatase activity.
To determine the potential relative contribution of each of these genes to inositol synthesis we carried out two experiments. One experiment looked at the relative amounts of mRNA using real-time RTq-PCR. All mRNA species were detectable, with cysQ being most abundant (approximately the same level as sigA, the major housekeeping sigma factor), and impA being the least abundant, with a level only one-tenth that of cysQ. We also assayed the level of IMPase activity in the whole cell extracts of each mutant, reasoning that we might see a decrease in activity when one of the genes was deleted. However, no decrease in activity was observed in any of the three mutants compared to the wild-type strain. This could be a reflection on the sensitivity of our assay, or could indicate that the activity is regulated (either at the transcriptional or post-transcriptional level) such that a constant level is maintained.
We also have preliminary data that expression of the impC gene is regulatable. We grew a Δino1 mutant of M. tuberculosis (which needs >50 mM inositol for its normal growth ) and looked at the effect of removal of the inositol on gene expression. The only IMPase gene with changed expression was impC, which was 3-fold increased. We cannot link this change directly to the inositol, because it could also be caused by the change in osmolarity, but at the very least indicates this indicates this gene is regulatable (unpublished results).
The situation with impC is complicated in that we could neither obtain a mutant, nor do we have biochemical evidence that it functions as an IMPase (despite many attempts to achieve both). The essentiality cannot be a simple case of impC producing the majority of the inositol in the cell, as we added inositol exogenously. It is true that the ino1 mutant we made previously, which is an inositol auxotroph, required levels of inositol approaching the maximum solubility limit, so a requirement for a slightly increased level of inositol might explain our findings. However, this is unlikely because (i) we also introduced a porin gene to increase inositol uptake, with no effect, (ii) we would also have to explain why the other three IMPase genes are not sufficient, and (iii) the level of impC mRNA is only 21% of the total IMPase mRNA (41% if cysQ is excluded). The only pieces of evidence we have, therefore, that link impC to inositol production are (i) its clear homology to IMPases, and (ii) the circumstantial evidence that levels of impC increased in a microarray experiment where inositol was removed from an ino1 auxotroph, whereas the expression level of the other IMPase genes was not significantly changed. We recognise the difficulty of carrying out the latter experiment in a controlled way since removing such a high level of inositol from the medium could have other effects. Interestingly, impC was also upregulated in the Wayne low oxygen model, particularly when M. tuberculosis cultures entered a microaerophilic state known as nonreplicating persistent stage 1 (NRP1), where there is cessation of bacterial replication, strong induction of respiratory nitrate reductase activity, and a change in energy metabolism (3.3-fold induced) .
We tested the hypothesis that the essentiality of impC is unrelated to its enzymatic activity by constructing a site-directed mutation. The mutation introduced changes at an active-site of glutamate to glutamine; the analogous mutation has been shown to abrogate activity in the human protein [40, 46]. Our inability to isolate mutants, strongly suggests that (i) the point mutation does indeed affect the activity of the enzyme and (ii) impC carrying this point mutation cannot complement a null mutant even in the presence of inositol. These findings oppose our hypothesis of a structural role for ImpC, and support an enzymatic role, as an explanation of its essentiality. There still remains a possibility that the mutation also affects the structure as we have not shown that folded protein is still produced, but we believe this is unlikely given the subtle nature of the change introduced. Another possible explanation for the inositol-independent essentiality is that removal of ImpC results in a build up of inositol-1-phosphate, which is somehow deleterious to the cell. However, we were unable to obtain an impC mutant in an ino1 background. It is feasible that ImpC uses a substrate other than inositol i.e. one involved in mycothiol production. The elegant work of Fahey and co-workers has defined most of the mycothiol biosynthesis pathway, but is missing a predicted phosphatase., which dephosphorylates N-acetyl glucosamine-(α1,3)-1L-inositol-1-phosphate. We carried out preliminary experiments attempting to make an impC mutant using this substrate (kindly provided by R. Fahey and G. Newton), without success (not shown). However, we have no evidence that it would penetrate the cell, so we feel we cannot draw any conclusions.
The impC gene lies upstream of the pflA gene and may be co-transcribed, as the intergenic gap is only 19 bp. PflA shows homology to pyruvate formate lyase-activating proteins; oxygen-sensitive iron-sulfur proteins that activate an anaerobic ribonucleotide reductase in some bacteria , although there does not appear to be a homologue to E. coli pyruvate formate lyase in the M. tuberculosis genome. We designed an unmarked deletion of impC, in order to prevent polar effects. In addition, complementation with impC alone was sufficient to allow mutants to be isolated. We have therefore excluded polar effects on pflA as an explanation for the essentiality.
The Mycobacterium leprae genome contains many pseudogenes therefore genomic comparisons may give an indication as to which mycobacterial genes are essential. In M. leprae, the impA orthologous gene is a pseudogene, with several frameshifts in the distal half of the gene, whereas the other three orthologous IMPase genes are retained. The suhB orthologous gene (ML1024) appears to be functional, and has a similar genomic context to the M. tuberculosis gene. The orthologous impC gene (ML0662) appears to be monocistronic in this species, and the orthologous cysQ gene (ML1301) is also present. The lack of phenotype in an M. tuberculosis impA mutant contrasts with the situation seen in M. smegmatis, where an impA mutant had altered colony morphology, slower growth, and reduced levels of PIM2 . The fact that the M. smegmatis mutant is viable supports the idea of some redundancy of function, and we suggest that the differences in phenotype are caused by different levels of ImpA compared to other IMPases in the two species.
Given that inositol monophosphatase and fructose-bisphosphatase activities were detected in cell extracts from impA, suhB and cysQ mutants, none of these genes can encode the major enzyme for these activities. The cysQ gene product does in fact act as a phosphatase with fructose-1,6- bisphosphate and inositol-1-phosphate , but enzyme activity in assays does not always equate to functionality in living bacteria. An example is found in Thermococcus kodakarensis where knocking out the fbp gene encoding a fructose bisphosphatase with high substrate specificity resulted in a strain unable to grow on gluconeogenic substrates whilst knocking out its imp gene encoding a member of the carbohydrate phosphate superfamily with substrate specificity including fructose-1,6- bisphosphate did not affect its growth on any carbon sources . In M. tuberculosis, the effect of knocking out the glpX gene that encodes fructose bisphosphatase is so drastic it is difficult to envisage that impA, suhB or cysQ can compensate for its loss .
We have demonstrated that the M. tuberculosis impA, suhB and cysQ genes are dispensable, but that impC is essential under the growth conditions used. The reason for the essentiality is unclear in terms of inositol synthesis; at present the most attractive hypothesis is that impC is required for mycothiol synthesis.
We thank Jane Turner for excellent technical assistance; Bob Cox for the suggestion to use mspA, Gerry Newton, Bob Fahey, Anne Lemassu, Philip Draper and Del Besra for helpful discussions, and Michael Niederweis and Claudia Mailaender for plasmid pMN013. FM was funded by the Wellcome Trust (project grant 051880) and the European Union TB vaccine cluster Contract no. QLK2-1999-01093 and Wellcome Trust grant 073237. PRW was funded by the Department for Environment, Food & Rural Affairs (UK), and (DEFRA). M. tuberculosis cosmids were kindly provided by Carol Churcher at the Sanger Centre.
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