- Research article
- Open Access
The analysis of para-cresol production and tolerance in Clostridium difficile 027 and 012 strains
© Dawson et al; licensee BioMed Central Ltd. 2011
- Received: 23 November 2010
- Accepted: 28 April 2011
- Published: 28 April 2011
Clostridium difficile is the major cause of antibiotic associated diarrhoea and in recent years its increased prevalence has been linked to the emergence of hypervirulent clones such as the PCR-ribotype 027. Characteristically, C. difficile infection (CDI) occurs after treatment with broad-spectrum antibiotics, which disrupt the normal gut microflora and allow C. difficile to flourish. One of the relatively unique features of C. difficile is its ability to ferment tyrosine to para-cresol via the intermediate para-hydroxyphenylacetate (p-HPA). P-cresol is a phenolic compound with bacteriostatic properties which C. difficile can tolerate and may provide the organism with a competitive advantage over other gut microflora, enabling it to proliferate and cause CDI. It has been proposed that the hpdBCA operon, rarely found in other gut microflora, encodes the enzymes responsible for the conversion of p-HPA to p-cresol.
We show that the PCR-ribotype 027 strain R20291 quantitatively produced more p-cresol in-vitro and was significantly more tolerant to p-cresol than the sequenced strain 630 (PCR-ribotype 012). Tyrosine conversion to p-HPA was only observed under certain conditions. We constructed gene inactivation mutants in the hpdBCA operon in strains R20291 and 630Δerm which curtails their ability to produce p-cresol, confirming the role of these genes in p-cresol production. The mutants were equally able to tolerate p-cresol compared to the respective parent strains, suggesting that tolerance to p-cresol is not linked to its production.
C. difficile converts tyrosine to p-cresol, utilising the hpdBCA operon in C. difficile strains 630 and R20291. The hypervirulent strain R20291 exhibits increased production of and tolerance to p-cresol, which may be a contributory factor to the virulence of this strain and other hypervirulent PCR-ribotype 027 strains.
- Surface Acoustic Wave
- Temporal Production
- Strain CA434
- Respective Parent Strain
Clostridium difficile is a spore forming Gram-positive anaerobe and is the leading cause of hospital-acquired diarrhoea worldwide [1, 2]. The hospital environment and patients undergoing antibiotic treatment provide a discrete ecosystem where C. difficile persists and selected virulent clones thrive. The recent upsurge in the number of C. difficile infection (CDI) cases has been linked to the rapid emergence of highly virulent and epidemic strains, known as PCR-ribotype 027. In the UK prior to 2005, 027 strains were rarely reported, but they now cause >33% of the 50,000 cases of CDI reported annually . Several studies have revealed that patients infected with PCR-ribotype 027 strains have more severe diarrhoea, higher mortality and higher level of recurrence [4–8]. This is exemplified by the strain R20291, a prototypical PCR-ribotype 027 strain responsible for the infection of over 160 patients at the Stoke Mandeville hospital, UK in 2004/2005 .
CDI characteristically occurs after treatment with broad-spectrum antibiotics. It is thought that antibiotic treatment disrupts the normal gut microflora, providing C. difficile with a competitive advantage to colonise the gut mucosa. The reason why C. difficile flourish under these conditions is unknown. Following colonisation, toxin production via TcdA and TcdB results in an acute inflammatory-response and severe damage to the intestinal epithelium . These two widely studied toxins are thought to be the main contributors to histopathology and disease burden. However, recent outbreaks of CDI in both Asia and Europe have been attributed to toxin defective (A-B+) strains and are generally PCR-ribotype 017 [11, 12]. This suggests that other factors are involved in C. difficile pathogenesis, survival and proliferation.
One of the relatively unique properties of C. difficile amongst anaerobes is its ability to produce p-cresol, a phenolic compound produced by the degradation of tyrosine via para-hydroxyphenylacetate (p-HPA) . Several studies have shown p-cresol is bacteriostatic and inhibits the growth of other bacteria . The production of p-cresol by C. difficile may provide the bacterium with a competitive advantage over the other gut microflora and facilitate the establishment of the pathogen. Furthermore, the organism itself must have inherent mechanisms to avoid or tolerate the toxic effects of p-cresol that may be linked with its ability to produce p-cresol. In C. difficile it has been hypothesised that p-cresol is produced via the oxidation of tyrosine to p-HPA followed by the decarboxylation of p-HPA to p-cresol . However, the temporal production of p-cresol and its relative production among different C. difficile strains have not been investigated. Genome sequencing of the strain 630 (PCR-ribotype 012) suggests that the p-HPA decarboxylase is encoded by three genes (CD0153-CD0155) designated hpdBCA . However, the genes involved in the conversion of tyrosine to p-HPA are unknown.
In this study we demonstrate the temporal and quantitative production of p-cresol by C. difficile in both minimal and rich media (supplemented with the intermediate p-HPA) using NMR spectroscopy and gas chromatography (zNose™). Gene inactivation mutations in the hpdA, hpdB and hpdC genes in strains 630Δerm and R20291 confirmed the absence of p-cresol production in all mutants tested and conclusively show that tyrosine is converted to p-HPA by C. difficile under minimal media growth conditions. We show that R20291 is more tolerant to p-cresol and has a higher capacity to convert tyrosine to p-HPA resulting in higher overall levels of p-cresol.
Para-cresol tolerance and production
Construction of gene inactivation mutants in C. difficile
Analysis of the decarboxylase mutants
Temporal production of p-HPA and p-cresol in mutant and parent strains
In this study we show two independent methods for measuring levels of p-cresol from C. difficile grown in vitro. NMR spectroscopy and gas chromatography (zNose™) provide a quantitative means of measuring the relative and temporal production of p-cresol by C. difficile. This revealed that that p-cresol is only produced from the conversion of tyrosine in minimal media. indicating that p-cresol production may be linked to the limitation of nutrients, or nutrient stress. However, the successful conversion of p-HPA to p-cresol in rich media suggests the limiting step in the cascade is the utilisation of tyrosine. Rich media may contain a constituent(s) such as glucose, which inhibits the conversion from tyrosine to p-HPA.
Gene inactivation mutations in the hpdB, hpdC and hpdA genes in strains 630Δerm and R20291 revealed the complete absence of p-cresol production in all mutants tested, confirming the role of the putative decarboxylase operon in p-cresol production in C. difficile. The build up of p-HPA observed in the hpdBCA operon mutants confirm that C. difficile converts tyrosine to p-HPA, rather than using an exogenous source of p-HPA and this conversion is significantly more efficient in R20291. With the exception of Clostridium scatologenes, the hpdBCA operon appears absent from the genomes of other sequenced anaerobic bacteria . The production of p-cresol coupled with its ability to produce tissue-damaging toxins may explain why C. difficile is almost unique among pathogens in causing antibiotic associated colitis. The production of p-cresol by C. difficile may provide a competitive advantage over other microorganisms during re-colonisation of the gut. If this hypothesis is true, C. difficile should itself be tolerant to the bacteriostatic properties of p-cresol. Previous studies have shown that in contrast to most other anaerobes, C. difficile is more tolerant to p-cresol . We have also shown that the modern hypervirulent 027 clonal lineage has a propensity to be more tolerant to p-cresol than other strains, as observed with BI-16, a recent 027 isolated which exhibits a level of tolerance similar to R20291. The historic 027 isolate CD196 exhibits a similar level of tolerance to strain 630 . This increase in tolerance to p-cresol in the modern hypervirulent 027 isolates may be linked to increased virulence.
In addition, the hypervirulent PCR-ribotype 027 strain has a higher capacity to convert tyrosine to p-HPA resulting in a higher overall yield of p-cresol. Analysis of the decarboxylase mutants revealed that although C. difficile can tolerate p-cresol, high levels have a deleterious effect on the growth rate of C. difficile, as the mutants grow better in-vitro than their respective parent strains. Although it is evident that the 027 ribotype R20291 is more tolerant to p-cresol and produces significantly more p-cresol than other strains, the mechanism of tolerance to p-cresol does not appear to be linked to its production. These results indicate that there is an intricate balance between optimal p-cresol production and deleterious effects on growth.
The hypervirulent R20291 strain produces high levels of p-cresol, and has an elevated tolerance, which may contribute to the colonisation and dissemination of the 027 clonal lineage by providing a selective advantage. There is a delicate interplay between relative p-cresol production and growth rate, whereby R20291 may have reached an advantageous compromise.
Bacterial strains and culture
C. difficile strains used in this study were 630, 630Δerm and R20291. Strain 630, PCR-ribotype 012, was originally isolated from a patient with severe PMC in Zurich, Switzerland in 1982. 630Δerm is an erythromycin sensitive strain that was isolated after passage of the original sequenced strain 630 . Erythromycin sensitivity is required for the construction of C. difficile gene inactivation mutants. R20291, a hypervirulent PCR-ribotype 027 strain was isolated from an outbreak at Stoke Mandeville hospital in 2006 and was provided by Jon Brazier (Anaerobe reference laboratory, Cardiff, UK). Strains were stored at -80°C and were cultured on BHI Agar (Oxoid), supplemented with 0.05% L-cysteine and cycloserine/cefoxitin antibiotic supplement (Fluka) at the recommended concentrations for 1 to 2 days under anaerobic conditions, in a Modular Atmosphere Control System 500 (Don Whitney Scientific) at 37°C. Liquid cultures were grown in BHI broth (Oxiod) supplemented with 0.05% L-cysteine and cycloserine/cefoxitin antibiotic supplement (Fluka) with and without 0.1% p-HPA (Sigma), or in yeast peptone (YP) broth, 16 gL-1 peptone (Sigma), 5 gL-1 yeast (Sigma), and 5 gL-1 NaCl2 (Sigma). E. coli strain CA434, the conjugation donor, was grown in Luria-Bertani (LB) broth or agar supplemented with 12.5 μg/ml chloramphenicol.
Para-cresol tolerance assays
Primary cultures were inoculated with three single colonies into pre-equilibrated media, shaking at 50 rpm on an orbital shaker. At an OD600 nm of 0.3-0.4, liquid cultures were inoculated 1/10 into pre-equilibrated media containing 0.05% (v/v) and 0.1% (v/v) p-cresol alongside an untreated control. These were incubated under anaerobic conditions for 4 hours before colony forming units were performed in pre-equilibrated 1 × PBS (Sigma), then plated in triplicate onto BHI plates and incubated for 24 hours under anaerobic conditions. CFU counts were determined for all of the test conditions and were calculated per ml of culture. The p-cresol stress CFU data was normalized to the untreated control and expressed as a percentage. Data was analysed in GraphPad Prism V4.02 using a two-tailed Student's t-tests with a p value cut off of p < 0.01.
Primary cultures of C. difficile were grown overnight as outlined above in either BHI broth, BHI supplemented with 0.1% p-HPA, or YP broth. Secondary cultures were inoculated 1/10 from the primary cultures into the relevant media. Samples were removed every hour up to 24 hours, the OD600 nm was taken and samples were double filter sterilized using 0.2 μM filter, then stored at -80°C.
1H NMR spectroscopy analysis was carried out to determine the production of p-cresol in rich media supplemented with p-HPA, and for determination of the temporal production of p-HPA and p-cresol in the mutant and wild-type strains to yield the relative levels of tyrosine and of the metabolites produced, p-HPA and p-cresol. Spectra were obtained using buffered extracts of the various cultures. Typically, 350 μl of sample was transferred to a 5 mm Norell HP507 NMR tube, and 150 μl of a pH 7.4 phosphate buffer with TSP added as a chemical shift reference was then added, providing a final sample volume of 500 μl.
All 1H NMR spectroscopy was carried out on a Bruker Avance-DRX600 instrument operating at 600.29 MHz, using a 5 mm TXI probe (Bruker BioSpin GmbH, 76287 Rheinstetten, Germany). The standard 1-D pulse sequence [RD-90°-t1-90°-tm-90°- acquire FID] was employed for all acquisitions, with water peak suppression achieved through irradiation of the water signal during tm and RD, using 8 dummy scans, a spectral width of 20.02 ppm, Fourier transform line broadening of 0.3 Hz, tm = 150 ms, and t1 = 3 μs. The first acquisition program for the rich media samples used 64 scans, 32 k time and frequency domain points, and a relaxation delay (RD) of 3.5 s. The second acquisition run for the temporal analyses employed 128 scans, and used a higher spectral resolution of 64 k time and frequency domain points, with a reduced relaxation delay (RD) of 2.137 s to maintain the across-acquisition quantitation status of the metabolites of interest. Within each run, the instrument receiver gain was set to a constant value for all samples.
The temporal metabolite profile analyses were carried out starting with Matlab R2008a (MathWorks Inc, Natick MA, USA), using proprietary in-house routines for some of the spectral import processing and for correlation analysis. Data was prepared and imported to Matlab initially using MetaSpectra over the spectral region between 0 and ~10.1 ppm, using 32 k data points, which is very close to the original acquisition digitisation density of 64 k over a 20.11 ppm sweep width. No spectral excision for the water residual signal region was made. Under the assumption of constant linewidth, relative quantitation for p-HPA and p-cresol in this work was based on peak heights for the higher shift peak from each doublet (6.875 and 6.838 ppm). Peak height quantitation under these assumptions has been shown to be a reliable quantitative approach . The TSP peak height and line width for the data array was used to verify this was a reasonable assumption, as well as confirming volumetric accuracy in sample preparation. This quantitation data was then placed into an Excel spreadsheet for calculation of the baseline corrected values, using the local baseline taken from the broth control samples having zero p-HPA and p-cresol present. Some STOCSY analysis of the data arrays (data not shown) was also used to confirm the conversion pathway sequence, by showing the appropriate anti-correlations in the levels of precursor and conversion metabolite . The metabolite quantitation data was then graphed using GraphPad Prism.
The zNose™ is an ultra rapid analytical device that allows real time monitoring of volatile compounds , by combining miniaturised gas chromatograph separation technology with a highly sensitive acoustic wave sensor. Primary and secondary cultures of C. difficile were set-up as outlined above and harvested at OD600nM 0.4 and at 24 hours, then these were transferred into pre-baked (overnight at 210°C) 40 ml glass vials sealed with screw caps with an integral PTFE/silicone septa (Supelco, Gillingham, UK).
Measurements were performed with a zNose™ Model 7100 bench top vapour analysis system (Electronic Sensor Technology, Newbury Park, CA) fitted with a capillary DB-624 column and a temperature controlled surface acoustic wave (SAW) detector. Headspace samples were withdrawn from the sealed vials via a side hole Luer needle inserted through the septum. Ten second samples were taken at a flow rate of 0.5 ml/second. All measurements were taken at ambient temperature. The column was ramped at from 40°C to 160°C at 10 C/s in a helium flow of 3.00 cm3. The SAW sensor operated at a temperature of 60°C and data were collected every 0.02 s. After each data sampling period the sensor was baked for 30 s at 150°C to remove any residual deposit and an air blank was run to ensure cleaning of the system and a stable baseline. On encountering compounds exiting the DB-624 column the SAW detector registers a depression in the frequency of the acoustic wave at its surface relative to a reference sensor. Derivativisation is performed automatically by the Microsense software (EST, Newbury Park, CA) and retention time and peak sizes are plotted. A reference sample of pure p-cresol (Sigma) was run under the same conditions to confirm that the retention time of the experimental peak observed (6.7 s) was identical to that of the target compound.
Production of gene inactivation mutants
List of oligonucleotides used in this study
List of plasmids used in this study
Commercial TA' cloning plasmid
ClosTron mutagenesis plasmid
Heap et al. 2007
pMTL007 carrying Ll.LtrB intron retargetted to hpdB
pGEM®-T Easy carrying Ll.LtrB intron retargetted to hpdC
pMTL007 carrying Ll.LtrB intron retargetted to hpdC
pGEM®-T Easy carrying Ll.LtrB intron retargetted to hpdA
pMTL007 carrying Ll.LtrB intron retargetted to hpdA
The retargeted intron was then cloned into the HindIII and BsrGI sites of pMTL007 to create the plasmids pLDhpdA2, pLDhpdB, and pLDhpdC2 (Table 2), which were transformed into the E. coli conjugation donor strain CA434 and transferred into C. difficile strains 630Δerm and R20291 by conjugation as previously described . Transconjugants were selected for in the presence of thiamphenicol (15 μg/ml, Sigma), after which mobilisation of the intron from the plasmid to the gene of interest was induced using IPTG. Screening for chromosomal insertion of the intron was performed with lincomycin (20 μg/ml, Sigma) for both C. difficile 630Δerm and R20291 to select for the restored ermB retrotransposition-activated marker (RAM) that signals integration into the genome. DNA was extracted for analysis from colonies, which were phenotypically lincomycin resistant, but thiamphenicol sensitive to indicate loss of the plasmid pMTL007. Potential mutants were verified by PCR, sequencing and Southern blot analysis.
Screening of mutants by PCR, sequencing and Southern blot
Potential mutants were screened by PCR, sequencing and Southern blot analysis to confirm the chromosomal integration of the intron within the desired genes and loss of the plasmid pMTL007. Three PCRs were performed to screen putative mutants using the following oligonucleotides (Table 1): i) RAM-F and RAM-R, to screen for loss of the group I intron, which insertionally inactivated the ermB RAM prior to chromosomal integration of the group II intron; ii) a gene specific primer and the group II intron specific EBS universal primer, to screen for insertion of the intron into the desired location in the genome; and iii) gene specific forward and reverse primers that flank the insertion site. Genomic DNA from C. difficile R20291 and 630Δerm, and plasmid DNA from pMTL007 were used as controls for the PCR reactions. PCR reactions were performed with GoTaq® PCR mix (Promega) in accordance with the manufacturers guidelines. The thermal cycling conditions were as follows: 95°C for 2 min × 1; 95°C for 30 sec, 50°C for 30 sec, 68°C for 8 min × 35 cycles; and 68°C for 10 min × 1.
Sequencing was performed across the junction of the gene to intron using gene specific primers and the EBS universal primer to verify insertion site. Southern blot analyses were performed using Roche DIG-High Prime DNA labelling and detection reagents, in accordance with the manufacturer's guidelines and visualised using CDP star (Roche). Genomic DNA from wild type and potential mutants was disgested with HindIII alongside plasmid DNA as a positive control. The probe was produced by PCR using SaII-R1 and EBS2 primers (Table 1), designed within the group II intron sequence.
This research was supported from the The Wellcome Trust (grant ref: 080860/C/06/Z). RHB acknowledges support from the BBSRC (CISBIC) and EC-FP7 FloriNASH (P22634).
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