Comparative transcription analysis and toxin production of two fluoroquinolone-resistant mutants of Clostridium perfringens
© Park et al; licensee BioMed Central Ltd. 2013
Received: 31 August 2012
Accepted: 18 February 2013
Published: 1 March 2013
Fluoroquinolone use has been listed as a risk factor for the emergence of virulent clinical strains of some bacteria. The aim of our study was to evaluate the effect of fluoroquinolone (gatifloxacin) resistance selection on differential gene expression, including the toxin genes involved in virulence, in two fluoroquinolone-resistant strains of Clostridium perfringens by comparison with their wild-type isogenic strains.
DNA microarray analyses were used to compare the gene transcription of two wild types, NCTR and ATCC 13124, with their gatifloxacin-resistant mutants, NCTRR and 13124R. Transcription of a variety of genes involved in bacterial metabolism was either higher or lower in the mutants than in the wild types. Some genes, including genes for toxins and regulatory genes, were upregulated in NCTRR and downregulated in 13124R. Transcription analysis by quantitative real-time PCR (qRT-PCR) confirmed the altered expression of many of the genes that were affected differently in the fluoroquinolone-resistant mutants and wild types. The levels of gene expression and enzyme production for the toxins phospholipase C, perfringolysin O, collagenase and clostripain had decreased in 13124R and increased in NCTRR in comparison with the wild types. After centrifugation, the cytotoxicity of the supernatants of NCTRR and 13224R cultures for mouse peritoneal macrophages confirmed the increased cytotoxicity of NCTRR and the decreased cytotoxicity of 13124R in comparison with the respective wild types. Fluoroquinolone resistance selection also affected cell shape and colony morphology in both strains.
Our results indicate that gatifloxacin resistance selection was associated with altered gene expression in two C. perfringens strains and that the effect was strain-specific. This study clearly demonstrates that bacterial exposure to fluoroquinolones may affect virulence (toxin production) in addition to drug resistance.
KeywordsClostridium perfringens Fluoroquinolone Resistance Toxin Virulence
Clostridium perfringens is commonly found in the gastrointestinal (GI) tract of humans, animals, soils, freshwater sediments and sewage. It can cause various diseases in humans, including food poisoning, antibiotic-associated diarrhea, sporadic diarrhea, internal abscesses, and gas gangrene and also various animal diseases [1–5]. C. perfringens strains all are prolific toxin producers and are classified based on their toxin formation. Various C. perfringens toxins denature cellular components of mammalian cells and are implicated in virulence and pathogenicity. Among these toxins are α-toxin (phospholipase C, PLC) and θ-toxin (perfringolysin O, PFO), which are essential for gas gangrene pathogenesis. Other toxins or hydrolytic enzymes may be involved in destruction of connective tissue or spread of bacteria in infected tissues [4, 6, 7]. C. perfringens, although a commensal, can cause life threatening infections and is implicated in inflammatory bowel diseases [8–10]. In a survey of Clostridium species bacteremia, in a Canadian hospital between 2000–2006, C. perfringens was shown to have caused 42% of the cases, which was more than any other Clostridium species . It causes nearly a million cases of food borne illness each year in the United States . Bacteria from the GI tract, including C. perfringens, may become resistant to fluoroquinolones used for treatment or prophylaxis of bacterial infections. Surveys of fluoroquinolone-resistant-anaerobes found ciprofloxacin-resistant C. perfringens as early as 1992 among clinical isolates . Although similar surveys have not been conducted in recent years, Gionchetti et al.  showed that treatment of patients with chronic treatment-resistant pouchitis with 1 g of ciprofloxacin for 15 days did not result in a statistically significant reduction in C. perfringens. One reason for fluoroquinolone resistance development is mutation in the fluoroquinolone target genes, gyrase (gyrA and gyrB) and topoisomerase IV (parC and parE) . Because fluoroquinolones are DNA-damaging agents, they may also induce the SOS response [14–16] that results in expression of DNA repair genes, which may lead to phenotypic changes in fluoroquinolone-resistant strains [17–20]. Excessive use of fluoroquinolones has been attributed to the emergence of virulent strains of bacteria [21–24]. Clostridium difficile strain NAP1/027, which emerged in 2002 in Canada and the USA, now has spread to most parts of Europe . In a gut model, higher rates of spore germination and levels of toxin production were observed in two ribotypes of C. difficile that were exposed to three different fluoroquinolones . Wide dissemination of virulent fluoroquinolone-resistant strains of Escherichia coli has been reported in East Asia . Other reports, sometimes conflicting, show either increased or decreased virulence in fluoroquinolone-resistant clinical isolates of bacteria [26–28]. Previously we showed that different C. perfringens strains rapidly developed resistance, even to high potency fluoroquinolones, and that resistant strains had various mutations in the fluoroquinolone target genes . In addition, the production of some enzymes was altered in some resistant mutants [30, 31]. One gatifloxacin-resistant strain, NCTR, had increased levels of α-toxin (phospholipase C, PLC) and θ-toxin (perfringolysin O, PFO) . These results point to global changes in the expression of various genes in gatifloxacin- resistant strains and to the need for further study. In this study, we have used genomic analysis (microarray and QRT-PCR) to compare the changes in gene expression in two gatifloxacin-resistant strains of C. perfringens following fluoroquinolone resistance selection, and have compared the toxin production and cytotoxicity of the strains. Strain NCTR was selected because of enhanced production of PLC and PFO by its gatifloxacin resistant mutant and was compared with strain ATCC 13124, which is a gangrene isolate whose genomic sequence is known, and its gatifloxacin resistant mutant 13124R has the same mutation in gyrA as NCTRR.
Growth of bacterial strains
Wild types and gatifloxacin-resistant mutants of C. perfringens strains ATCC 13124 and NCTR  were used in this study. The development of these mutants (Gat-13124-10 and Gat-NCTR- 10) was described previously . Both mutants have stable mutations in target genes and will be referred to as 13124R and NCTRR in this study. Both mutants had a mutation in gyrA (G81C, D87Y), 13124R had mutation in gyrB (A431S) and parC (S89I), and NCTRR had a mutation in parE (E486K). The bacteria were grown anaerobically under an atmosphere of 85% N2, 10% CO2, and 5% H2 at 37°C in brain heart infusion (BHI) broth (Remel, Lenexa, KS) with vitamin K (1 μg/ml), hemin (5 μg/ml), and L-cysteine (5 μg/ml) (Sigma Chemical Co., St. Louis, MO) . No antibiotics were added.
Preparation of RNA
Early exponential (2.5-3.0 h) growth phase cultures of all four strains, grown in BHI under identical anaerobic conditions, were used to isolate RNA for microarrays. Cells from 100-ml cultures were harvested by centrifugation (15,000 × g, 10 min, 4° C), washed with 10 mM Tris and 1 mM EDTA (pH 8.0), and suspended in 1 ml of buffer containing 10 mg/ml of lysozyme (Sigma). The mixtures were incubated for 10 min at room temperature and centrifuged (15,000 × g, 10 min, 4° C). The samples were suspended in 0.5 ml TE (10 mM Tris, 1 mM EDTA) and mixed with 5 ml of RNA-Bee isolation reagent from TEL-TEST, Inc. (Friendship, TX). After addition of 1 ml chloroform to the mixture, the samples were incubated on ice for 30 min and centrifuged (15,000 × g, 30 min, 4° C). The clear phases were harvested, added to an equal volume of isopropanol and centrifuged to pellet the RNA. The RNA was further purified using an RNeasyR Mini Kit (50) from QIAGEN, Inc. (Valencia, CA), according to the instructions provided with the kit. After RNA extraction and purification, contaminating DNA was removed using 10 U of RNase-free DNase 1 (Boehringer Mannheim, Ingelheim, Germany). The quantity and quality of total RNA was determined using a Nanodrop ND-1000 spectrophotometer (NanoDrop Technology, Wilmington, DE). RNA purification steps for real-time PCR (qRT- PCR) were essentially the same. The RNA was stored at −80° C and used within a week to avoid degradation of RNA. RNA was extracted from three different cultures of each strain for microarray analysis and qRT-PCR.
Probe design for microarrays
The probes were designed by Biodiscovery LLC, Ann Arbor, MI (http://www.mycroarray.com/) from the sequences of C. perfringens strains 13 (CPE) and ATCC 13124 (CPF in http://www.ncbi.nlm.nih.gov), using OligoArray v 3.1 (http://berry.engin.umich.edu). The designs of microarrays were submitted to MIAMExpress and can be accessed at the following links: for strain 13124, [http://www.ebi.ac.uk/arrayexpress/arrays/A-MEXP-2008], and for strain NCTR, at [http://www.ebi.ac.uk/arrayexpress/arrays/A-MEXP-2027].
The microarrays were hybridized by Biodiscovery LLC to fluor-labeled RNA at 60° C for at least 16 h in 2-gasket slides and commercial hybridization chambers (Agilent, Santa Clara, CA) while being rotated (~4 rpm) in a hybridization incubator. The hybridization solution contained 6 × SSPE (1 M NaCl, 50 mM NaH2PO4, 50 mM Na2HPO4, 3 mM EDTA, pH 6.7), 1 μg/μl acetylated BSA, 1 μg/μl herring sperm DNA (Promega, Madison,WI), 0.01% Tween 20 (Sigma) and 10 μg template RNA per array. The hybridized arrays were washed twice in 6 × SSPE for 5 min at 60° C, once in 1 × SSPE for 5 min at 20° C, and once in 0.25 × SSPE at 20° C for 1 min, and then were spun dry in a microarray high-speed centrifuge (ArrayIT, model MHC). The arrays were scanned in an Axon 4000B scanner (Molecular Devices Sunnyvale, California), controlled by GenePixPro software (v 184.108.40.206). The resulting images were quantified with the same software and the results were archived in the gpr file format. The mean expression of each gene for the mutant was divided by the mean expression of the same gene for the wild type. Those genes for which the values were ≥ 1.5 were considered upregulated in the mutant, and the genes for which this value was ≤0.6 were considered downregulated in the mutant. The genes that were upregulated or downregulated were selected for further RT-PCR analysis.
Quantitative real-time PCR (qRT-PCR)
Primers used for qRT-PCR are listed in Additional file 1. The genes that were upregulated in one mutant and downregulated in the other mutant, in comparison with their respective wild types, by microarray analysis were selected to design primers. Some genes involved in regulation of transcription were also selected. The sequence of C. perfringens ATCC 13124 (http://www.ncbi.nlm.nih.gov/nuccore/CP000246.1) was used to design primers that generated PCR amplicons of 100–150 bp in length via the default setting of “Primer 3 Input software” (http://frodo.wi.mit.edu/primer3). For cDNA template synthesis, SuperScriptTM III First-Strand Synthesis SuperMix (Invitrogen, Carlsbad, CA) was used. For qRT-PCR, SYBR® GreenERTM qPCR SuperMix (Invitrogen) was used. The reaction mixtures were prepared on ice according to the manufacturer’s instructions. Each reaction contained 2 × Express SYBR Green ER qRT-PCR universal mix, 25, 2.5, or 0.25 ng of the cDNA template, and 2 μM each of the forward and reverse primers. The amplification was performed using a CFX96 Real-Time PCR detection system (Bio-Rad, Hercules, CA) and the following protocol: 50° C for 10 min, 95°C for 8.5 min to inactivate uracil DNA glycosylase and activate DNA polymerase, followed by 40 cycles of 95°C for 15 s and 60°C for 1 min to amplify cDNA. Melting curves were monitored at 65-95°C (1°C per 5 s) to detect any nonspecific amplification. Either 25, 2.5, or 0.25 ng of each 16S rRNA gene was amplified as a reference RNA of equivalent size for normalization . Reaction mixtures without reverse transcriptase, for detecting genomic DNA contamination, and reaction mixtures without templates, for detecting nucleic acid contamination of reagents and tubes, were included as controls. Each PCR reaction was run in triplicate for each type of RNA isolated from three different cultures of each wild type or mutant. The relative level of mRNA expression was calculated by the 2-ΔΔCT method according to Real-Time PCR Application Guide (Additional file 2).
Detection of phospholipase C (PLC) and perfringolysin O (PFO)
PLC and PFO activities were measured according to the methods previously described [7, 30, 33]. The hemoglobin release from red blood cells in the presence of perfringolysin buffer was measured to detect perfringolysin O (PFO) according to the method of O'Brien and Melville . The increase in turbidity of lecithin in egg yolk emulsion or the release of nitrophenol from O-(4-nitrophenyl-phosphoryl) choline as the result of hydrolysis by PLC was used to measure phospholipase C (PLC) activity [7, 30].
The amounts of collagenase in the mutants and wild types were calculated by the method of Awad et al.  by measuring the amount of dye released from Azo Dye Impregnated Collagen (azocoll) (Sigma). Azocoll powder was washed and resuspended in 0.2 M of borate buffer (pH 7.2) containing 0.15 M NaCl, 20 μM ZnCl2 and 5 mM CaCl2 to a final concentration of 5 mg azocoll per ml. Next, 100 μl of the filter-sterilized supernatants of centrifuged wild types and mutants were added to 400 μl of azocoll solution and the mixtures were incubated for 2 h at 37° C. Following centrifugation at 16,100 × g, the released dye was measured by the absorbance at 550 nm.
Assay for clostripain
A clostripain substrate, N-carbobenzoxy-L-arginine p-nitroanilide (Z-Arg-pNA) (Bachem Americas, Torrance, CA), was used for measuring the amounts of clostripain in the supernatants of wild types and mutants . The filter-sterilized supernatant from each centrifuged strain was incubated overnight at 4°C in a buffer containing dithiothreitol to reduce the thiol group of the cysteine residues of clostripain. Next, 20 μl of the sample was added to the 300 μl buffer containing 2 mM CaCl2 and 260 mM of Z-Arg-pNA. The kinetics software of the spectrophotometer was programmed to measure the absorbance at 410 nm every min for 30 min. The amount of cleavage of Z-Arg-pNA was measured and the enzyme units were calculated. One unit was defined as the amount of enzyme that hydrolyzed 1.0 μmol of Z-Arg-pNA per min .
Detection of sialidase
Sialidase activity was measured in filter-sterilized supernatants of centrifuged cultures of mutants and wild types, using 4 mM 5-bromo-4-chloro-3-indolyl-α-D-N-acetylneuraminic acid, sodium salt . The assay reaction was performed in 96-well plates by addition of the supernatant to wells containing the substrates, according to a procedure recommended by Sigma for measuring recombinant C. perfringens neuraminidase. The kinetics software was programmed to measure the absorbance at 595 nm.
The amounts of hyaluronidase in the filter-sterilized supernatants of centfifuged wild types and mutants were quantified by measuring the degradation of hyaluronic acid. Bovine hyaluronic acid (Sigma) was dissolved in acetate buffer (200 mM sodium acetate, 150 mM NaCl, pH 6.0) to a final concentration of 1 mg/ml. 100 μl of the hyaluronic acid solution was incubated with 400 μl of the filter-sterilized supernatants of the wild types and mutants for 30 min at 37° C. One ml of a solution containing 2% NaOH and 2.5% cetramide (cetyltrimethylammonium bromide, Sigma) was added to the reaction mixture. The turbidity of the insoluble complex formed between cetramide and hyaluronic acid was measured at 400 nm . The reduction in turbidity, reflecting the decrease in hyaluronic acid because of the activity of hyaluronidase, was calculated by comparing the turbidities of samples containing the supernatant of each culture with controls containing BHI alone. The enzyme assays for all the enzymes were performed three times from three different cultures of each strains.
Cytotoxicity of C. perfringens supernatants for macrophages
Macrophages were obtained from C57BL/6 male mice, 4–6 weeks old, which had ad libitum access to food and water. The maintenance, handling and sacrifice of mice were according to procedures approved by the NCTR Institutional Animal Care and Use Committee. Resident mouse peritoneal macrophages were harvested by peritoneal lavage, using 4 ml of supplemented DMEM medium, containing 5% heat-inactivated fetal bovine serum, 100 μg/ml streptomycin sulfate, 100 units/ml penicillin G, 110 mg/L sodium pyruvate, and 2 mM glutamine. Red blood cells were removed by hypotonic lysis. The peritoneal exudate cells were washed once with DMEM, plated and incubated at 37°C in a humidified atmosphere of 5% CO2. Floating cells were removed and the macrophages were incubated in DMEM, containing 10% BHI or filter-sterilized supernatants of overnight cultures of wild types and mutants, for 18 h at 37°C in a CO2 incubator. A CytoTox 96® Non-Radioactive Cytotoxicity Assay Kit (Promega) was used to measure the toxicity of the mutants and wild type cultures for macrophages. The cytotoxicity of each absorbance unit of the cells of different strains was calculated by the amount of lactate dehydrogenase (LDH) released from the macrophages. The differences in cytotoxicity due to the mutants and wild types were assessed using Student’s t-test.
Colony morphology of the strains was compared after overnight growth on BHI plates. For cellular morphology, log phase grown cells were Gram stained and examined under the light microscope.
Several regulatory and toxin genes and enzymes from wild types and mutants were amplified and sequenced as previously described .
Transcriptional analysis by DNA microarray
Microarray and qRT-PCR analysis of the genes that were differentially affected in the gatifloxacin resistant mutants, NCTR R and 13124 R
Gene ID and name
putative membrane protein
CPE0162 CPF_0155 (pfoR)
putative membrane protein
CPE0278 CPF_0274 (sagA)
putative monogalactosyl-diacylglycerol synthase
CPE0036 CPF_0042 (plc)
CPE0846 CPF_0840 (cloS1)
CPE1474 CPF_1725 (hlyC)
CPE0163 CPF_0156 (pfoA)
CPE0782 CPF_0784 (ahpC)
alkyl hydroperoxide reductase-C subunit
CPE1092 CPF_1348 (pac)
choloylglycine hydrolase family protein
CPE1299 CPF_1505 (eno)
CPE2058 CPF_2315 (gadB)
CPE2437 CPF_2747 (nrdH)
glutaredoxin-like protein, YruB-family
CPE2551 CPF_2875 (glpA)
probable glycerol-3-phosphate dehydrogenase
Purines, pyrimidines, nucleotides, and nucleosides
CPE2276 CPF_2558 (guaB)
CPE2622 CPF_2958 (purA)
CPE0173 CPF_0166 (colA)
CPE2323 CPF_2632 (pepF)
probable oligoendopeptidase F
CPE1205 CPF_1002 (abgB)
amidohydrolase family protein
putative regulatory protein
CPE1533 CPF_1784 (scrR)
sucrose operon repressor
CPE2035 CPF_2292 (hrcA)
heat-inducible transcription repressor HrcA
two-component sensor histidine kinase
Transport and binding proteins
CPE1240 CPF_1450 (mgtE)
CPE1300 CPF_1507 (gadC)
glutamate:γ-aminobutyrate antiporter family protein
CPE1505 CPF_1756 (uraA)
ABC transporter, ATP-binding protein
CPE0761 CPF_0756 (gltP)
sodium:neurotransmitter symporter family protein
CPE2084 CPF_2341 (modB)
molybdate ABC transporter, permease protein
CPE2343 CPF_2652 (malE)
putative maltose/maltodextrin ABC transporter
nitroreductase family protein
CPE1784 CPF_2038 (nifU)
NifU family protein
PSP1 domain-containing protein
Microarray analysis of the genes that were upregulated in one or both gatifloxacin-resistant mutants, 13124 R and NCTR R
Gene ID and name
Amino acid biosynthesis
branched-chain amino acid aminotransferase
capsular polysaccharide biosynthesis protein
UDP-glucose/GDP-mannose dehydrogenase family
putative membrane protein
putative membrane protein
putative membrane protein
ATP synthase epsilon subunit
ATP synthase beta subunit
ATP synthase alpha subunit
ATP synthase delta subunit
ATP synthase B chain
ATP synthase C chain
Fatty acid and phospholipid metabolism
3-oxoacyl-(acyl-carrier-protein) synthase III
malonyl CoA-acyl carrier protein transacylase
3-oxoacyl-(acyl-carrier-protein) synthase II
acetyl-CoA carboxylase, biotin carboxyl carrier
beta-hydroxyacyl-(acyl-carrier-protein) dehydratase FabZ
acetyl-CoA carboxylase, biotin carboxylase
acetyl-CoA carboxylase, carboxyl transferase, beta subunit
acetyl-CoA carboxylase, carboxyl transferase, alpha subunit
ribosome recycling factor
ribosomal protein L7AE family
ribosomal protein L34
Purine, pyrimidine, nucleotides, and nucleosides
Transport and binding proteins
conserved hypothetical protein
Microarray analysis of the genes that were downregulated in both gatifloxacin-resistant strains, 13124 R and NCTR R
Gene ID (name)
Biosynthesis of cofactors, prosthetic groups, and carriers
4-hydroxy-3-methylbut-2-enyl diphosphate reductase
carbohydrate kinase family protein
CPF_0721 (nanI) *
ethanolamine utilization protein, EutP
Purine, pyrimidine, nucleotides, and nucleosides
purine nucleoside phosphorylase
transcriptional regulator, DeoR family
probable PBP5 synthesis regulator protein
transcriptional regulator, PadR family
transcriptional regulator, PadR family
probable transcriptional regulator
Transport and binding proteins
amino acid ABC transporter
PTS system, sucrose-specific IIBC component
putative maltose/maltodextrin ABC transporter
degV family protein
mutator mutT protein homolog
phnA family protein
Validation of DNA microarray data by qRT-PCR
Results of qRT-PCR for the C. perfringens regulatory genes in the wild types and mutants
Gene ID and name
DNA binding response regulator, VirR
sensor histidine kinase, VirS
conserved hypothetical protein
GTP-sensing transcriptional pleiotropic repressor CodY
DNA binding response regulator
Toxin production in the mutants and wild types
Cytotoxic effects on mouse peritoneal macrophages
Gram staining of log phase cultures showed that gatifloxacin resistance selection affected the shape of cells (Additional file 4). As expected, the Gram reaction was positive for both wild types and their mutants. The resistant mutants were more elongated than the wild types but the amounts of elongation and differences in cell shape were much more pronounced for the NCTR/NCTRR strain pair than for the ATCC 13214/13124R strain pair. Fluoroquinolone resistance selection also affected the colony morphology of the resistant strains. The colony size of NCTRR was bigger than that of the wild type, and the colony size of 13124R was smaller than that of the wild type (Additional file 4).
The use of fluoroquinolones has been listed as a risk factor for the emergence of virulent antibiotic-resistant strains of some bacteria [21–23]. We studied the effect of fluoroquinolone resistance selection on the global transcriptional response in gatifloxacin-resistant C. perfringens strains 13124R and NCTRR by microarray analysis. The fluoroquinolone resistance selection resulted in alteration of transcription levels of a significant number of genes involved in almost every aspect of metabolism in the resistant mutants of both strains in comparison with their wild types. Many genes with similar functions were either upregulated or downregulated in the resistant mutants. However, some genes that were downregulated in 13124R were upregulated in NCTRR. qRT-PCR analysis confirmed that the transcription of these genes, which included toxin genes for phospholipase C (PLC), perfringolysin O (PFO), collagenase and clostripain, were affected differently in the two mutants. Similarly, the production of these enzymes and the toxicity of the culture supernatants decreased in 13124R and increased in NCTRR. It appears that gatifloxacin resistance selection resulted in alteration of global gene transcription in C. perfringens and that the effect was strain-specific.
The changes in the levels of global gene expression due to the response to fluoroquinolone exposure may be governed by complex regulatory processes. Both resistant strains harbored some common and some unique mutations in fluoroquinolone target genes. These enzymes are involved in the DNA supercoiling process that plays an essential role during gene transcription [38, 39]. Although neither of the resistant strains was a clinical isolate, some of the mutations found in the resistant strains were the same as those found in fluoroquinolone-resistant mutants of E. coli obtained from clinical samples, which were also the same as those found in fluoroquinolone-resistant mutants of E. coli generated in the laboratory [29, 40].
The expression of a number of genes is affected by supercoiling  and aberrant expression of these genes occurs when DNA supercoiling has been altered by gyrase mutation(s). Alleles of gyrA that reduce DNA supercoiling have been shown to generate metabolic defects and reduce fitness of gyrase mutant strains [38, 41]. Furthermore, because fluoroquinolones are DNA-damaging agents, in addition to inducing mutation in target genes, changing DNA superhelicity, they may also induce the expression of DNA repair genes via the SOS response, which may lead to phenotypic changes [15, 17–20]. Cirz et al.  characterized the global transcription response of S. aureus to ciprofloxacin and, among other changes, found induction of the SOS response, upregulation of the TCA cycle and downregulation of α-hemolysin and a leukocidin family toxin. The positive regulators of transcriptional responses for stress and toxin genes were also downregulated . In C. perfringens, although the expression of several virulence genes decreased in one resistant mutant (13124R), it increased in another (NCTRR). The transcription of various genes, including toxin genes, is regulated by virR and virS[32, 42, 43]. VirS is a sensor histidine kinase, which autophosphorylates in response to extracellular signals, and VirR is a response regulator [32, 42, 43]. These two genes, along with vrr (which is an RNA regulator virR-RNA), are implicated in controlling gene transcription  and were upregulated in NCTRR. In 13124R, transcription of VirR did not change, and virS and vrr were downregulated. The gene vrr is directly regulated by VirR/VirS, and as a regulatory RNA, controls transcription of 147 genes, including housekeeping and toxin genes, in C. perfringens[32, 44]. Obana et al.  showed that VR-RNA regulates the stability of colA mRNA by cleaving the transcript. The processed shorter colA transcript was more stable than the longer intact colA transcript. It is possible that among other factors, downregulation of vrr in 13124R (−158) may have contributed to a decrease in the level of transcription of genes. The vrr in NCTRR was upregulated twofold. virX is another regulatory gene that, even in the absence of the VirR/VirS regulatory system, activates the transcription of the pfoA, plc and colA genes, and its overexpression results in the increased expression of toxin genes [44, 46]. qRT-PCR results showed that the expression of this gene increased at least 2.2 times in NCTRR and decreased by −3.0 in 13124R.
Another regulatory gene whose expression was altered in the mutants was revR, which was downregulated in 13124R and upregulated in NCTRR. revR is a response regulator that alters the transcription of 100 genes, including those for potential virulence factors, which also are regulated by (VirR/VirS), and those for cell wall metabolism . Hiscox et al.  found that a revR mutant of C. perfringens 13 was filamented. Gram staining of the wild types and mutants of ATCC 13124 and NCTR showed that cells of both mutants were filamented and longer than those of the wild types. Microarray and qRT-PCR analysis (Table 1) showed that some putative membrane protein genes were differentially expressed in the mutants and wild types of both strains.
The amino acid sequences of the toxin genes and the regulatory genes (virR/virS) in the mutants and wild types of both strains were identical, except that there were two silent mutations in virR/virS in NCTRR, so the expression of toxin genes and their regulators was not the result of gene mutation. The sequence of vrr was identical in the mutants and wild types of both strains, and the sequence of revR in ATCC 13124 and 13124R was also identical. Obana and Nakamura  also detected other regulatory genes, CPE_1446-CPE_1447, which appear to regulate the transcription of plc, pfoA, nanI and nagHIJK at transcription level. Microarray analysis showed that CPE_1447 was downregulated in NCTRR, but this gene was not detected in the microarray data from ATCC 13124. qRT-PCR confirmed that nanI was downregulated and sialidase was decreased in NCTRR; however, the role of CPE_1447 in the regulation of this gene is not clear.
Another global regulatory protein, CodY, has been shown to regulate expression of many genes in Bacillus subtilis and Clostridium difficile[49, 50]. It appears to repress genes whose products are not needed during growth in high nutrient medium. qRT-PCR showed that CodY was upregulated (6.9 times) in NCTRR and downregulated (−1.89 times) in 13124R. The sequence of codY was identical in both ATCC 13124 and 13124R. Since both mutants and wild types were grown in a rich medium, the effect of CodY on alteration of gene expression in our strains is not known.
In addition, microarray analysis also detected some regulatory genes that were downregulated in both mutants (Table 3) and some that were upregulated in NCTRR and downregulated in 13124R (Table 1). Among those genes that were affected differently was CPF_0069, which is a transcription antiterminator similar to the BglG-type regulators in other bacteria (http://www.ncbi.nlm.nih.gov/). This gene was downregulated in 13124R and upregulated in NCTRR. At this point, the roles that this gene and others play in altering the transcription of toxin genes in resistant strains are not known. Nor is there a reason known for the contradictory effects of fluoroquinolone resistance selection on the expression of regulatory genes, including those that regulate toxin production, and it needs to be investigated further. Autoinducers (AI-2) also have been implicated in the regulation of some toxin genes . However, in our strains, the production of AI-2 per cell unit, measured by the indicator Vibrio harveyi, was higher for 13124R than for ATCC 13124 and lower for NCTRR than for NCTR. The ratio of AI-2 production per OD unit in an overnight culture of the mutant to that of the wild type was 1.5 for ATCC 13124 and 0.14 for NCTR. The contradictory results observed in the transcription of various toxin genes in two resistant strains were accompanied by changes in the levels of toxins and other enzymes. The most dramatic changes were observed for phospholipase C (PLC) and perfringolysin O (PFO). These two toxins were substantially decreased in 13124R and increased in NCTRR. The alterations in the production of enzymes were accompanied by changes in cytotoxicity for macrophages. The cytotoxicities of cell-free culture supernatants of the wild type ATCC 13124 and NCTR, for the macrophages were comparable. However, the cell-free culture supernatant of 13124R exhibited significantly lower cytotoxicity for macrophages than ATCC 13124, but that of NCTRR had higher cytotoxicity than NCTR. These data were consistent with the alterations in the transcription patterns of toxin genes and enzyme assays that were observed by DNA microarray analysis, qRT-PCR assay and toxin production. The cytotoxic effects were correlated with the transcription pattern of toxins and virulence-associated genes and enzymatic activities, confirming that the effect of fluoroquinolones on C. perfringens was strain-specific. O’Brien and Melville  reported that perfringolysin O (PFO) plays a more prominent role than α-toxin (PLC) in cytotoxicity for macrophages. Since we used the crude extract, which contains various factors including PFO and PLC, our results only show the alteration in the overall cytotoxicities of the mutants in comparison with their wild types and the contributing factors and their affinities for macrophage receptors are not known. Fluoroquinolone resistance selection decreased the toxicity of 13124R and increased the toxicity of NCTRR.
Our study demonstrates that gatifloxacin resistance selection in C. perfringens was associated with upregulation or downregulation of different genes involved in various aspects of metabolism and that the effect was strain-specific. The genes involved in transcription regulation, virulence and cell toxicity were among those that were upregulated in one resistant strain and downregulated in another. Hiscox et al.  surmised that “the regulation of virulence in C. perfringens was a complex process” and we found that the nature of each strain adds yet another level of complexity to gene regulation in C. perfringens. Myer et al.  found widely variable large genomic islands in a large collection of C. perfringens strains and stated that considerable variation exists among the genomes of C. perfringens strains. It appears that this variation in gene structure of different C. perfringens strains also affects gene regulation and interaction of bacteria with fluoroquinolones. Fluoroquinolones have been implied to have a role in the development of C. difficile associated diarrhea . Since virulent, drug-resistant clinical isolates of pathogenic bacteria have an undefined genetic basis for their resistance and virulence, we used two wild types and otherwise isogenic resistant mutants, which are difficult to obtain in a clinical setting, to assess fluoroquinolone effects. Our results reflect clinical observations of finding fluoroquinolone-resistant strains of bacteria that are more or less virulent than the susceptible strains. They underscore the role of fluoroquinolones in changing bacterial virulence and the importance of prudent use of fluoroquinolones. Further study is needed on the effect of fluoroquinolones on a larger number of C. perfringens strains, along with genomic analysis of the resistant mutants.
- gyrA and gyrB:
- parC and parE:
Brain Heart Infusion
VirR, virX, vrr(VR-RNA), Cody RevR: Regulatory genes.
We thank Drs. Mark Hart and John B. Sutherland for their helpful comments on the manuscript, Dr. Carl E. Cerniglia for support of research and Drs. Donald Schwartz and Jean-Marie Rouillard for DNA microarray experiments. S.P. was supported by the FDA Commissioner’s Fellowship Program. The views presented in this article do not necessarily reflect those of the US Food and Drug Administration.
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