The protein profile of dormant Mtb obtained after the gradual acidification of Mtb culture was studied to find antigenic proteins for humans that are expressed by M. tuberculosis (Mtb) cells in vitro under conditions close to the situation of persistence in vivo. According to 2D electrophoresis, a significant diversity of proteins in dormant cells was found. However, the representation of individual proteins in dormant versus active cells differed substantially. Immunoblotting in different protein fractions of dormant cells revealed ten proteins that are able to bind antibodies in pooled sera of TB patients. Two proteins (Rv2018 and Rv0341) are new immunogenics that were not previously found in other studies. Four proteins (Rv0341, Rv2018, Rv1509, Rv2986) with the maximal structural specificity for Mtb due to their unique extended domains were selected for further analysis. These proteins were expressed in E. coli cells and studied via enzyme-linked immunosorbent assay (ELISA) for the immunogenicity of individual sera of TB patients and healthy donors. All proteins were found to have the ability to react with individual sera of TB patients. In TB patients, 5–45% (depending on the particulate protein) have a titer that is higher than the average titers of healthy donors +SD; the most immunogenic was protein Rv2986. Thus, the application of phenotypically changed (dormant) Mtb cells makes it possible to identify a specific repertoire of immunodominant proteins that could be used in the construction of polypeptides that are useful for the serodiagnosis of active/latent TB.
Tuberculosis (TB) remains a deadly infectious disease. Each year, about 10 million people fall ill from TB, and 1.5 million die (https://www.who.int/news-room/fact-sheets/detail/tuberculosis). Although the main epidemiological figures for tuberculosis have stabilized over the past years in the Russian Federation, the epidemic of tuberculosis is still spreading in Russia. In 2019, the Russian Federation was among the twenty countries with the most unfavorable situations for TB (https://www.who.int/news-room/fact-sheets/detail/tuberculosis). The situation is complicated by the high and growing levels of the detection of TB strains resistant to first-line antibiotics (up to 29% in 2018) . Another concern regarding the epidemiology of tuberculosis is the high incidence of latent TB infection; an estimated one-quarter of the world’s population is latently infected, according to the WHO. Some epidemiologists believe that about 80% of the Russian population is latently infected with Mycobacterium tuberculosis (Mtb). However, the detection of such forms is difficult, since the TB bacteria remain inactive (dormant) in the body during latent infection; these bacteria remain “non-culturable” (NC) and need to be reactivated in order to be cultured.
Despite significant progress in our understanding of the mechanisms underlying latent tuberculosis, many aspects of the long-term persistence of the pathogen in the host body remain a mystery. Apparently, the interaction between the pathogen and the host, in particular, the interaction with the host immune system, plays a significant role in this process . Therefore, it is relevant to reveal a repertoire of immunogenic proteins in dormant forms (DFs) of Mtb, which differ considerably by their biochemical composition from those detected in active multiplying bacteria [3, 4].
In addition, the identification of immunodominant proteins in Mtb DFs may be of interest for the selection of antigens relevant to TB serodiagnosis. It is noted that such selection is usually based on our knowledge of the production of Mtb proteins during active growth, which is very different from the real situation of Mtb persistence in the host body. Evidently, successful serodiagnosis requires knowledge of the repertoire of Mtb antigens expressed in vivo under the influence of stress on the pathogen, e.g., factors of the host immune system. Herein, Mtb DFs, which form in response to the action of stress conditions on bacterial cells in vitro, can represent a unique model of the pathogen state for the study of the Mtb antigen pool in situations that are close to in vivo. Hence, fundamental research regarding stress-related proteomics of mycobacteria is needed.
The goal of this work is to identify immunodominant Mtb proteins expressed in an experimental model of stressed cells in vitro with methods of proteomics and immunology.
Formation of dormant M. tuberculosis cells. The wild-type Mtb strain H37Rv (obtained from the Central Tuberculosis Research Institute, Moscow) was studied. The strain was initially grown on standard Sauton’s medium (g/L): KH2PO4, 0.5; MgSO4⋅7H2O, 1.4; L‑asparagine, 4.0; trivalent ferric ammonium citrate, 0.05; sodium citrate, 2.0; 1% ZnSO4, 0.1 mL, glycerol, 60 mL; рН = 7.0 (adjusted with 1 М NaOH). ADC supplement (bovine serum albumin, glucose, and NaCl) and Twin-80 (0.05%) were added .
Dormant, NC mycobacteria that lost the ability to grow on solid media due to gradual acidification of the medium during the stationary growth phase were obtained as described earlier . The bacteria were grown for 12–15 days in 50 mL of Sauton’s medium with the addition of 0.05% Twin-80 and ADC in 100-mL flasks on an orbital shaker (200 rpm). These bacterial cultures were used for passage to a modified Sauton’s medium to obtain NC Mtb. The modification of the Sauton’s medium included the replacement of Twin-80 to 0.025% tyloxapol and ADC to 0.5% bovine serum albumin, Cohn Analog (Sigma, United States). In contrast to standard Sauton’s medium (at a pH of 7.0), the initial pH values in the modified media were 6.2. The modified Sauton’s medium (200 mL) was placed into a 500-mL flask (three to five flasks per experiment) and incubated at 37°C for 40–60 days with stirring. The pH of the medium was measured periodically. When the pH reached 6.0–6.2 in the stationary phase, the cultures were transferred to closed, plastic, 50-mL tubes, and 2-(N-morpholino)ethanesulfonic acid (MES) was added to a final concentration of 20 mM to prevent subsequent acidification during long-term storage. Incubation was continued under static conditions at room temperature in the dark for 1 year after seeding.
2D-electrophoresis. Active and dormant cells obtained in four biological repeats of the experiment as described above were combined. The quantity of cells comprised approximately 3.5 g of wet mass. The bacterial culture was centrifuged at 7000 rpm for 15 min and washed ten times with a buffer containing the following (g/L): NaCl, 8; KCl, 0.2; Na2HPO4, 0.24 (pH 7.4). The cellular pellet was resuspended on ice in a 100-mM HEPES (4-(2-hydroxyethyl)piperazine ethanesulfonic acid) buffer at a pH of 8.0 containing protease inhibitor cocktail (Sigma, United States) and phenylmethylsulfonyl fluoride (PMSF); the cells were then disrupted with zirconium beads and a FastPrep-24 homogenizer (MP Biomedicals, United States) for 1 min five times for active cells and ten times for dormant cells. The lysate was centrifuged at 13 000 g for 15 min at 4°C. The supernatant was divided into membrane (sediment) and cytosolic fractions (supernatant) via ultracentrifugation at 100 000 g for 2 h based on the principles of sedimentation.
The membrane fraction was washed three times with HEPES buffer via ultracentrifugation and isolated via extraction with sodium dodecyl sulfate detergent (2% sodium dodecyl sulphate (SDS)).
The cytosolic fraction and membrane extract were precipitated with a ReadyPrep 2-D purification kit (BioRad, United States) for the selective precipitation and removal of contaminants, such as detergents, lipids, and phenolic compounds, from the protein samples. This precipitation procedure made it possible to resuspend the protein precipitate in an isoelectrofocusing buffer containing 8 M urea, 2 M thiourea, 10 mM 1,4-dithiotreitol (DTT), 2 mM tris(2-carboxyethyl)phosphine hydrochloride (TCEP), 1% (wt/vol) CHAPS, 1% (wt/vol) Triton X-100, 1% (wt/vol) amidosulfobetaine-14 (ASB), and 0.4% (vol/vol) ampholytes (pH 3–10).
Isoelectric focusing was performed in 5% polyacrylamide gel (PAAG) (30% acrylamide/bisacrylamide, 8 M urea, 2% ampholytes, pH 3–10 and 4–6 (1 : 4), 1% CHAPS, 1% Triton X-100, 0.4% ASB) in glass tubes with an inner diameter of 2.4 mm in an isoelectrofocusing cell (Tube Cell 175, BioRad, United States) until it reached 3700 volt-hours.
A total of 100 µg of protein from each sample was used for analysis. After isoelectric focusing, the gels were extracted from the glass tubes and fixed in buffer 1 (0.375 М tris-HCl, рН 6.8, 2 М urea, 20% (vol/vol) glycerol, 2% SDS, 2% DTT) and buffer 2 (0.375 М tris-HCl, рН 6.8, 2 М urea, 20% glycerol, 2% SDS and 0.01% bromophenol blue) for 15 min each. The second direction was carried out as described by O’Farrell  with large plates (20 × 20 cm) in 12% PAAG gels with SDS 1.5 mm thick in standard tris-glycine buffer in PROTEAN II xi cell for vertical electrophoresis (BioRad, United States). The gels were stained with Coomassie CBBG-250 (Roti-Blue Carl Roth, Germany), followed by silver staining (https://www.alphalyse.com/wp-content/uploads/2015/09/Silver-stained-protocol.pdf).
The gel images were obtained with Syngene G: BOX Gel & Blot Imaging Systems (Syngene, United Kingdom). The images of Coomassie stained gels were analyzed with the TotalLab TL120 software to calculate the spot density.
Each visible protein spot corresponding to the spot on immunoblot was manually cut from the gel and analyzed as a separate specimen via matrix-assisted laser desorption ionization time-of-flight (MALDI-TOF) analysis. After MALDI-TOF, tandem mass spectrometry (MS/MS) data were used to search the Mascot Protein database (MSDB) for protein identification. The protein functions were taken from the Tuberculist database. Each specimen for 2D analysis was checked twice.
MALDI-TOF protein analysis. Proteins stained with Coomassie brilliant blue on polyacrylamide gels were digested with trypsin as follows. A piece of gel 3–4 mm3 in size was washed twice in 100 µL of 40% acetonitrile solution in 0.1 M NH4HCO3 for 20 min at 37°C to remove the dye.
Proteins stained with silver on PAAG gels were hydrolyzed as follows. A 3- to 4-mm3 piece of gel was washed twice in 100 µL of a mixture containing 30 mM K3Fe(CN)6 and 100 mM Na2S2O3 (1 : 1) for 15 min to remove the dye. After the liquid phase was removed, it was washed three times with deionized water for 10 min. After the removal of the dye, the gel was washed with 40% acetonitrile solution in 0.1 M NH4HCO3 for 20 min.
After the washing solutions were removed, acetonitrile (100 µL) was added to dehydrate the gel. After acetonitrile was removed and a piece of the gel was dried, 3.5 µL of modified trypsin solution (Promega, United States) in 0.05 M NH4HCO3 in a concentration of 15 mg/mL was added. Hydrolysis was performed for 5 h at 37°C; 5.25 µL of 0.5% TFA in a 50% solution of aqueous acetonitrile was added and thoroughly mixed. The solution on the gel was used to obtain the MALDI mass spectra.
The sampels for mass spectrometry were prepared as follows: 1.5 µL of the sampel and 0.5 µL of a 2,5-dihydroxybenzoic acid solution (10 mg/mL in 20% aqueous acetonitrile, 0.5% TFA) were mixed on the target, and the resulting mixture was air-dried.
Mass spectra were generated with an Ultraflextreme MALDI-TOF mass spectrometer (Bruker, Germany) equipped with a UV laser (Nd). Measurements were performed in positive ion reflectron mode. The accuracy of the measured monoisotopic mass peaks upon additional calibration after trypsin autolysis was 0.007% (70 ppm). Spectra were obtained in the mass range of 500–6500 m/z with the selection of the optimal laser power to achieve the best resolution. Fragmentation spectra were obtained with the tandem MS mode. The mass accuracy measurement of the fragment ions was at least 2 Da.
The proteins were identified with the Blast tool of the National Center for Biotechnology Information (NCBI). Candidate peptide sequences were selected from the proteins of other organisms based on the assumed amino-acid sequences for the fragmentation spectra of individual peptides. The mass spectra were processed with the FlexAnalysis 3.3 software (Bruker Daltonics, Germany).
Immunoblotting. Immunoblotting was performed after the proteins were transferred from the gels to the PVDF membrane in a Protean chamber (Bio-Rad, United States). The reaction of the primary antibodies was carried out in a solution containing antibodies from patients or healthy people (dilution 1 : 300), 5% bovine serum albumin, and 0.1 M NaCl for 1 h. The membranes were washed with the same solution without antibodies three times for 10 min. Hybridization with secondary antibodies was performed with peroxidase-conjugated, goat, antihuman antibody (Sigma-Aldrich, United States) diluted in a ratio of 1 : 20 000. After secondary antibodies were washed off, the spots were visualized with BCIP (5-bromo-4-chloro-3-indolyl phosphate) and NBT (nitro blue tetrazolium chloride) (Sigma-Aldrich, United States) according to the manufacturer’s recommendations.
Preparation of recombinant proteins. The genes encoding Rv0341, Rv2018, Rv1509, Rv2986, Rv0432, and Rv3676 proteins were cloned from the genomic DNA of the M. tuberculosis H37Rv strain with the primers F 5'-GGCACGcatatgACCTCGCTTATCG-3' (small letters indicate NdeI restrictase recognition site) and R 5'-GCGTAggatccAGATCACGGTATGC-3' (BamHI site is indicated) for the Rv0341 gene; F 5'-GTGAATcatatgGCTGGCGACC-3' (NdeI site is indicated) and R 5'-GctcgagGATTCCGATCAGGCT-3' (XhoI site is indicated) for the Rv2018 gene; F 5'-catatgGTGTTTGCGTTGAGTAATAATCTG-3' (NdeI site is indicated) and R 5'-ggatccTTACCTCTTCGTTAGCCGCAC-3' (BamHI site is indicated) for the Rv1509 gene, F 5'-ATCcatatgATGAACAAAGCAGAGCTCATT-3' (NdeI site is indicated) and R 5'-CATggatccCTATTTGCGACCCCGCCGAGC-3' (BamHI site is indicated) for the Rv2986 gene; F 5'-ATCggatccATGCCAAAGCCCGCCGATCAC-3' (BamHI is indicated) and R 5'-CATTaagcttGCCGGAACCAATGACACCGCA-3' (HindIII is indicated) for the Rv0432 gene; F 5'-ATCgaattcGTGGACGAGATCCTGGCCAGG-3' (EcoRI is indicated) and R 5'-CATTaagcttCCTCGCTCGGCGGGCCAGTCT-3' (HindIII is indicated) for the Rv3676 gene.
The PCR products of the Rv0341 and Rv1509 genes were ligated to the pGEM-T easy intermediate vector (Promega, United States) and then transferred to the pET19b final plasmid. The coding part of the Rv2018 and Rv2986 genes was cloned directly into the pET19b vector without intermediate steps. The Rv0432 and Rv3676 genes were cloned in the pET23a vector. The constructs were transformed into an expression strain of E. coli BL21DE3. The expression of recombinant proteins from the plasmids led to protein synthesis with a polyhistidine tag (10 Нis) at the N-end of the polypeptide (pET19b vector) and with a polyhistidine tag (6 Нis) at the C-end of the polypeptide (pET23a vector). Both intermediate and final genetic constructs were verified via PCR and sequencing.
For each protein, the isolation and purification conditions were optimized via metallo-chelate chromatography under denaturing conditions. To obtain protein, an individual colony was inoculated into 50 mL of meat peptone broth (MPB) containing 100 µg/mL of ampicillin. The culture was incubated overnight with stirring (220 rpm) at 37°C. Afterwards, 200 mL of MPB medium (two to four flasks with 200 mL of the medium) containing 100 µg/mL of ampicillin was inoculated with 1% of the night culture; the expression inducer isopropyl-β-D-thiogalactoside (IPTG, 1 mM) was added when the optical density of the culture reached OD600 0.5–0.6. Subsequent incubation was performed with stirring at 37°C or at room temperature (cold induction) for 4–5 h. At a low level of protein expression, induction was carried out overnight. Cells were collected via centrifugation at 4000 g for 15 min and resuspended in 5 mL of a buffer containing 5 mM imidazole, 0.5 M NaCl, 20 mM tris-HCl, pH 8.0 (buffer 1x BB), in the presence of 8 M urea. The cell biomass was stored at –20°C for 2–4 weeks.
DNase (5 units) and RNase (5 µg) were added to the thawed cell biomass in the presence of Mg2+ (5 mM) and 1х ВВ, pH 8.0 (1 × ВВ, pH 9.0 was added to the recombinant Rv1509 protein). The cell biomass was disrupted with an ultrasonic disintegrator (three to five times for 1 min) and centrifuged at 10 000 g twice for 30 min at 4°C. The supernatant was loaded onto a column with Ni2+-NTA-sepharose 6B equilibrated with 1 × ВВ. After the specimen was loaded, the column was washed with 10 volumes of 1 × BB.
The protein was obtained in two stages. In stage 1, the urea concentration was reduced from 8.0 M to 0 (urea gradient) over 40 min. In stage 2, the protein was eluted with 5–500 mM imidazole (in steps) for 1 h 20 min.
Each recombinant protein was dialyzed with an appropriate buffer. The Rv0341 protein was dialyzed with a buffer containing 10 mM Na2HPO4, 5 mM NaCl, pH 8.0. The Rv1509 protein was dialyzed with a buffer containing 25 mM Tris-HCl, 250 mM NaCl, pH 9.0. The Rv2018 protein was dialyzed with a buffer containing 20 mM Tris-HCl, 200 mM NaCl, pH8.0. The Rv2986, Rv0432, and Rv3676 proteins were dialyzed with a buffer containing 40 mM Tris-HCl, 150 mM NaCl, pH 8.0. The proteins were dialyzed twice at 4°C. The proteins were filtered through Millex-GV and Millipore 0.22 µm (Sartorius, Germany) and stored at 4°C.
The protein concentrations were measured with the Flores method  and/or a spectrophotometer (BioDrop, Germany) according to the absorption ratio at 280 and 260 nm with allowance for the molar extinction coefficient.
The purity of recombinant proteins was evaluated via 12% PAAG electrophoresis and immunoblotting with specific anti-His antibodies and confirmed via MALDI.
Measurement of the protein concentration with the Flores method. A dye solution (0.9 mL, 0.0075% bromophenol blue solution, 15% ethanol, and 2.5% acetic acid) was added to 0.1 mL of the analyzed protein solution. The optical density was measured via spectrophotometry at 610 nm. Bovine Serum Albumin (BSA) was used to construct the calibration curve. Each sample was analyzed in three repeats.
Determination of the immunoglobulin concentration in blood serum with ELISA. Sorption of the antigen was performed in the wells of a Costar 96-well plate (United States) with a high binding surface overnight at 4°C from 100 µL of solution with a concentration of 1.0 µg/mL in a 10 mM phosphate buffer, pH 7.4, with 0.17 M NaCl (FBS). The well plates were washed four times with a phosphate buffer containing 0.05% twin-20 (FBS-T); 100 µL of sera diluted with FBS-T at a starting dilution of 1 : 50 and standards of affinity isolated human anti-TB antibodies (0 to 1000 µg/mL) were then added to the wells and incubated for 30 min at 37°C. The well plate was washed three times; 100 µL of a solution of monoclonal antihuman IgG-peroxidase labeled antibodies in FBS-T (1 : 1000) were added and incubated for 30 min at 37°C. After three washings of the well plate, the enzyme immunoassay reaction was assessed in each well. For this, 100 µL of 50 mM citrate-acetate buffer, pH 5.2, with 0.035% 3,3',5,5'—tetramethylbenzidine, and 0.01% Н2О2, were added to the wells and incubated for 15 min at room temperature; the reaction was stopped with 1.0 M H2SO4, and the OP was measured at 450 nm. The concentration of the bound immunoglobulins was estimated with a calibration curve constructed based on human anti-TB antibody standards.
RESULTS AND DISCUSSION
To detect immunoreactive proteins in Mtb cells in a state close to in vivo conditions, we used dormant Mtb cells that formed during long-term cultivation with gradual acidification of the culture medium in the poststationary stage . It is known that acidification of the medium is a main factor limiting the growth of M. tuberculosis pathogens in macrophages . Cytosolic and membrane fraction proteins were extracted from M. tuberculosis cells obtained during acidification of culture medium, as well as from active multiplying Mtb cells. The protein profiles were obtained via 2D electrophoresis . Despite the long-term storage of dormant cells without division, the proteome of such cells retained a large quantity of proteins, but individual proteins differed from the proteome of active cells. Protein stability may be associated with the presence of a substantial number of enzymes involved in protection against oxidative stress, as well as chaperones. The proteome of dormant Mtb cells included enzymes involved in specific metabolic pathways that may provide low-level metabolism, or these proteins may be stored for use during reactivation prior to the upregulation of biosynthetic processes .
Immunoreactive proteins in stressed Mtb cells were detected via immunoblotting of the proteins (active and dormant mycobacteria) obtained after 2D electrophoresis. The isolated immunoglobulins from the pooled serum of TB patients were used as primary antibodies. Incubation with secondary antibodies led to the appearance of stained spots. The corresponding protein spots on the original gel were cut out and identified via MALDI-TOF analysis. As a result, nine proteins were detected in dormant cells, and 21 were found in active cells (Table 1). It is notable that these proteins differed in active and dormant cells, except for three proteins, Rv1475c, Rv3804c, Rv1886c.
Sequence alignment of immunoreactive proteins from dormant Mtb to protein sequences of other bacteria with the BLAST tool made it possible to rank these proteins based on their similarity with proteins of other bacteria, except for the members of the M. tuberculosis complex (score parameter, Table 2). The three proteins with the lowest score value, i.e., possessing the highest structural specificity for Mtb due to the presence of extended domains unique to Mtb, were subsequently studied in more detail. The corresponding genes were cloned to obtain recombinant proteins (Rv0341 is isoniazid-induced protein IniB; Rv1509 is a protein with unknown function; Rv2018 is an antitoxin) in the form of His-tag proteins based on the pET19b expression vector system (Novagen, India). The recombinant proteins were able to bind specific anti-His-tag antibodies during 12% PAAG electrophoresis and immunoblotting (Fig. 1). Their correspondence to the original proteins was confirmed via MALDI-TOF (not shown).
The recombinant proteins were tested via immunoblotting for their ability to bind antibodies from the sera of TB patients. Immunoglobulins isolated via affinity chromatography from the pooled sera of 12 TB patients were used as primary antibodies. It was found that the best results were observed if the lipoproteins were preliminary precipitated from serum with dextran sulfate in the presence of calcium ions. The secondary antibodies were phosphatase-conjugated, antihuman antibody or peroxidase conjugated protein G. Incubation led to the appearance of stained bands corresponding to protein spots on the original gel. The immunoreactivity of these recombinant proteins was checked with the use of two additional panels of pooled sera from TB patients. In immunoblotting, all three proteins were capable of binding serum antibodies (Fig. 2).
Since it was possible that not all proteins (especially hydrophobic or oligomeric ones) could be detected via 2D electrophoresis, 1D SDS PAAG gel electrophoresis of proteins was used to separate the proteins of dormant cells. Immunoblotting of the proteins after this separation revealed an immunoreactive band with a high activity in the region of 20 kDa. In MALDI-TOF, three proteins were revealed in the immunoreactive area: Rv2986c, hupB (a DNA-binding protein of the HU family); Rv0432, sodC (periplasmic copper- and zinc-cofactored superoxide dismutase); Rv3676, crp, (a transcriptional regulator protein that belongs to Crp/Fnr protein family). To identify an immunoreactive protein, all three genes were cloned in E. coli cells, and the corresponding proteins were obtained as recombinant proteins in the pET vector system (pET19в and pET23а). The obtained individual proteins were subjected to denaturing PAAG electrophoresis, and immunoblotting with pooled sera from TB patients was performed. It was found that the Rv2986с protein was the only protein capable of binding serum immunoglobulins (Fig. 3). This protein was studied in subsequent experiments.
The obtained four recombinant proteins were used to evaluate the presence of antibodies in individual sera of TB patients and healthy donors via ELISA.
In total, four series of experiments were conducted (one for each protein). In each experiment, 42 sera from TB patients and 42 sera from healthy donors were used. The data revealed that all four recombinant antigens were recognized by the sera of TB patients (Fig. 4). However, only 5–45% of patients (for different antigens) had immunoglobulin concentrations that exceeded the average values for healthy donors. The maximal elevation was shown for the Rv2986 protein concentration. At the same time, antibodies at concentrations exceeding the same average value were also detected in the sera of 2–14% of healthy donors.
Two of the studied proteins (Rv2018 and Rv0341) are novel and had not been previously described in the literature. The Rv2018 protein was similar to an antitoxin from the VapB family, which is found in G/C-rich actinobacteria, including mycobacteria. It is thought that the toxin–antitoxin systems are essential for the entry of a bacterial population to a dormant state . Based on BLAST, the protein encoded by the Rv0341 gene (isoniazid inducible gene protein, IniB) is revealed exclusively in mycobacteria and occurs within large complexes (680 kDa or larger) in the membrane extract of dormant M. tuberculosis cells. These complexes decay to a monomeric form in an early reactivation stage of dormant mycobacteria, and large Rv0341 protein complexes disappear in the logarithmic phase. The IniB protein colocalizes with nucleic acids in membrane extracts of dormant mycobacteria . IniB is found to be overexpressed when macrophages are infected with Mtb cells. Fragments of the IniB protein bind well to the Major Histocompatibility Complex (MHC) on class 1 and 2 lymphocytes, and, hence, IniB appears to be involved in the cellular immunoresponse . According to a recent publication, IniB protein demonstrates good protective efficacy against TB infection . However, IniB protein was not previously described as possessing the ability to bind antibodies, and it was not included in the list of immunogenic proteins obtained during studies of the total immunoproteome from active Mtb cells in publications in 2010–2020 [13–15]. The protein encoded by the Rv2986c gene is a DNA-binding protein and is a histone-like protein (HupB, HU-homolog). Its expression is increased both in the stationary phase of Mtb growth and in a hypometabolic state [16–18]. The immunogenic HupB found in the cell wall fraction of active Mtb was described earlier in the literature . It was also found that the concentration of antibodies to this protein or HupB fragments in the sera of TB patients significantly exceeds that of healthy donors [20, 21]. However, these data were not confirmed in studies of the total immunoproteome in active Mtb cells. Such studies evaluated the immunogenicity for most proteins of the Mtb proteome [13, 15]. For example, in a 2010 study  of the total pool of Mtb proteins, 484 proteins were found to be recognized by patient sera; they did not include the proteins identified in our study (including HupB). Of the 484 proteins, the 13 proteins most often recognized by individual sera were isolated. However, the immunogenicity of proteins even in this group varied significantly among patients with TB. A similar large variability in immunogenicity was described in a recent publication on TB serodiagnosis in 755 patients from several countries with a panel of 22 Mtb antigens preselected from the total proteome in the form of recombinant proteins , as well as in a work on the identification of biomarkers for the serodiagnosis of latent TB .
The fact that the antigens selected in our study were not found in the publications cited above may be due to the methods used to express a large number of proteins with special protein microarrays that do not cover 100% of the Mtb proteome , in which the purity of the expressed proteins is not achievable . Such an approach differs from the expression of individual proteins, for which experimental selection was carried out and immunogenic proteins were identified with the use of in vitro models similar to the one used our study, which, hence, represents a promising direction.
In general, the use of this approach made it possible to identify immunodominant Mtb proteins, including novel ones not been previously described in the literature that demonstrate the ability to bind antibodies in the sera of TB patients. Since dormant Mtb cells were investigated in this study, it cannot be excluded that presence of antibodies in sera to the detected immunodominant proteins is associated with persistence of the Mtb pathogen in the host body.
In both the cited works and our study, the quantity of antibodies to individual antigens varies significantly in TB patients. It is thought that this may occur for several reasons, including (1) the occurrence of most pathogen cells in a different metabolic and physiological state in a particular patient and, hence, the different expression of a given antigen at the time of blood sampling; (2) the genetic characteristics of the patients and the associated features of the immunoresponse, which may also affect the synthesis of antibodies; and (3) the average, low level of humoral response in TB patients (especially in chronic infection), which leads to variability in the quantity of antibodies to a specific antigen [13, 14]. Conversely, antibodies that react with the same antigens are detected in the sera of some healthy people. This may be due to the presence of nonspecific Mtb domains in the primary structure of the studied proteins. A study of the immunoreactivity of polypeptides constructed based on the specific protein domains revealed in this study may be promising in terms of TB serodiagnosis.
Nechaeva, O.B., Tuberk. Bolezni Legk., 2018, vol. 8, no. 96.
Apt, A.S., Logunova, N.N., and Kondratieva, T.K., Tuberculosis, 2017, vol. 106, pp. 1–8.
Shleeva, M.O., Kudykina, Y.K., Vostroknutova, G.N., Suzina, N.E., Mulyukin, A.L., and Kaprelyants, A.S., Tuberculosis, 2011, vol. 91, no. 2, pp. 146–154.
Trutneva, K.A., Shleeva, M.O., Demina, G.R., Vostroknutova, G.N., and Kaprelyans, A.S., Front. Cell. Infect. Microbiol., 2020, vol. 10, p. 26.
Connell, N.D., Methods Cell Biol., 1994, vol. 45, pp. 107–125.
O’Farrell, P.H., J. Biol. Chem., 1975, vol. 250, pp. 4007–4021.
Flores, R., Anal. Biochem., 1978, vol. 88, pp. 605–611.
Welin, A., Raffetseder, J., Eklund, D., Stendahl, O., and Lerm, M., J. Innate Immun., 2011, vol. 3, no. 5, pp. 508–518.
Barer, M.R. and Harwood, C.R., Adv. Microb. Physiol., 1999, vol. 41, pp. 93–137.
Shleeva, M., Trutneva, K., Shumkov, M., Demina, G., and Kaprelyants, A., FEBS Open Bio, 2018, vol. 8, no. S1, p. 400.
Flyer, D.C., Ramakrishna, V., Miller, C., Myers, H., McDaniel, M., Root, K., Flournoy, C., Engelhard, V.H., Canaday, D.H., Marto, J.A., Ross, M.M., Hunt, D.F., Shabanowitz, J., and White, F.M., Infect. Immun., 2002, vol. 70, no. 6, pp. 2926–2932.
Bettencourt, P., Muller, J., Nicastri, A., Cantillon, D., Madhavan, M., Charles, P.D., Fotso, C.B., Wittenberg, R., Bull, N., Pinpathomrat, N., Waddell, S.J., Stylianou, E., Hill, A., Ternette, N., and McShane, H., NPJ Vaccines, Springer US, 2020, vol. 5, no. 2. https://doi.org/10.1038/s41541-019-0148-y
Kunnath-Velayudhan, S., Salamon, H., Wang, H.Y., Davidow, A.L., Molina, D.M., Huynh, V.T., Cirillo, D.M., Michel, G., Talbot, E.A., Perkins, M.D., Felgner, P.L., Liang, X., and Gennaro, M.L., Proc. Natl. Acad. Sci. U. S. A., 2010, vol. 107, no. 33, pp. 14703–14708.
Broger, T., Basu, RoyR., Filomena, A., Greef, C.H., Rimmele, S., Havumaki, J., Danks, D., Schneiderhan-Marra, N., Gray, C.M., Singh, M., Rosenkrands, I., Andersen, P., Husar, G.M., Joos, T.O., Gennaro, M.L., Lochhead, M.J., Denkinger, C.M., and Perkins, M.D., Clin. Infect. Dis., vol. 64, no. 7, pp. 947–955.
Peng, Z., Chen, L., and Zhang, H., J. Int. Med. Res., 2020, vol. 48, no. 3. https://doi.org/10.1177/0300060520910042
Matsumoto, S., Furugen, M., Yukitake, H., and Yamada, T., FEMS Microbiol. Lett., 2000, vol. 182, no. 2, pp. 297–301.
Matsumoto, S., Yukitake, H., Furugen, M., Matsuo, T., Mineta, T., and Yamada, T., Microbiol. Immunol., 1999, vol. 43, no. 11, pp. 1027–1036.
Lewin, A., Baus, D., Kamal, E., Bon, F., Kunisch, R., Maurischat, S., Adonopoulou, M., and Eich, K., BMC Microbiol., 2008, vol. 8, p. 91.
Yeruva, V.C., Duggirala, S., Lakshmi, V., Kolarich, D., Altmann, F., and Sritharan, M., Clin. Vaccine Immunol., 2006, vol. 13, no. 10, pp. 1137–1142.
Sritharan, N., Choudhury, M., Sivakolundu, S., Chaurasia, R., Chouhan, N., Rao, P.P., and Sritharan, M., Eur. J. Clin. Microbiol. Infect. Dis., 2014, vol. 34, no. 1, pp. 33–40.
Sivakolundu, S., Mannela, U.D., Jain, S., Srikantam, A., Peri, S., Pandey, S.D., and Sritharan, M., Trans R Soc. Trop. Med. Hyg, 2013, vol. 107, no. 1, pp. 43–50.
Zhou, F., Xu, X., Wu, S., Cui, X., and Pan, W., BMC Infect. Dis., 2017, vol. 17, no. 1, p. 793.
This study was conducted with the facilities of the Industrial Biotechnologies Center for Common Use (Bach Institute of Biochemistry, Fundamentals of Biotechnology Federal Research Center).
This study was supported by the Russian Science Fund (grant no. 16-15-00245-P). The Rv0341 recombinant protein was obtained with the support of the Russian Foundation for Basic Research, project no. 18-015-00239.
Conflict of Interests. The authors declare that they have no conflict of interest.
Statement of Compliance with Standards of Research Involving Humans as Subjects. All procedures performed in studies involving human participants were in accordance with the ethical standards of the institutional and/or national research committee and with the 1964 Helsinki Declaration and its later amendments or comparable ethical standards. Informed consent was obtained from all individual participants involved in the study.
Translated by M. Novikova
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Trutneva, K.A., Avdienko, V.G., Demina, G.R. et al. Immunoreactive Proteins of Dormant Mycobacterium tuberculosis Cells. Appl Biochem Microbiol 57, 170–179 (2021). https://doi.org/10.1134/S0003683821020174
- M. tuberculosis
- dormant forms
- enzyme-linked immunosorbent assay