Community-associated Clostridium difficile infection (CDI) appears to be an increasing problem. Reported carriage rates by C.difficile are debatable with suggestions that primary asymptomatic carriage is associated with decreased risk of subsequent diarrhoea. However, knowledge of potential reservoirs and intestinal carriage rates in the community, particularly in the elderly, the most susceptible group, is limited. We have determined the presence of C.difficile in the faeces of a healthy elderly cohort living outside of long-term care facilities (LCFs) in the United Kingdom.
Faecal samples from 149 community-based healthy elderly volunteers (median age 81 years) were screened for C.difficile using direct (Brazier's CCEY) and enrichment (Cooked Meat broth) culture methods and a glutamate dehydrogenase (GDH) immunoassay. Isolates were PCR-ribotyped and analysed for toxin production and the presence of toxin genes.
Of 149 faecal samples submitted, six (4%) were found to contain C.difficile. One particular sample was positive by both the GDH immunoassay and direct culture, and concurrently produced two distinct strain types: one toxigenic and the other non-toxigenic. The other five samples were only positive by enrichment culture method. Overall, four C.difficile isolates were non-toxigenic (PCR-ribotypes 009, 026 (n = 2) and 039), while three were toxigenic (PCR-ribotypes 003, 005 and 106). All individuals who had a positive culture were symptom-free and none of them had a history of CDI and/or antibiotics use in the 3 month period preceding recruitment.
To our knowledge, this is the first study of the presence of C.difficile in healthy elderly community-dwelling individuals residing outside of LCFs. The observed carriage rate is lower than that reported for individuals in LCFs and interestingly no individual carried the common epidemic strain PCR-ribotype 027 (NAP1/BI). Further follow-up of asymptomatic carriers in the community, is required to evaluate host susceptibility to CDI and identify dynamic changes in the host and microbial environment that are associated with pathogenicity.
Citation: Miyajima F, Roberts P, Swale A, Price V, Jones M, Horan M, et al. (2011) Characterisation and Carriage Ratio of Clostridium difficile Strains Isolated from a Community-Dwelling Elderly Population in the United Kingdom. PLoS ONE 6(8): e22804. doi:10.1371/journal.pone.0022804
Editor: Markus M. Heimesaat, Charité, Campus Benjamin Franklin, Germany
Received: December 23, 2010; Accepted: July 6, 2011; Published: August 23, 2011
Copyright: © 2011 Miyajima et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by the Liverpool Biomedical Research Centre (Royal Liverpool University Hospital/NHS Trust and the Wolfson Centre for Personalised Medicine/University of Liverpool), the National Institute for Health Research and The Northwest Development Agency. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
In the last decade, there has been an upsurge in the prevalence and severity of Clostridium difficile infection (CDI) such that it has become a major healthcare problem . This has coincided with the emergence of more virulent epidemic strains, particularly PCR-ribotype 027 (NAP1/BI) that have caused hospital outbreaks in North America and Europe with high morbidity and mortality . There is growing evidence for the existence of significant functional differences between epidemic and non-epidemic historical types from isolates of the same ribotype/toxinotype group , , possibly associated with a strong selective pressure due to broad antimicrobial usage. Community-associated CDI appears to be adding to this disease burden , although this may have been underreported.
Relatively little is known about potential community reservoirs and intestinal carriage rates of C. difficile in individuals living outside health care facilities. In neonates, for example, the carriage frequency is significantly higher than in any adult group , . Although neonates rarely develop CDI, they may act as important reservoirs and there is evidence of cross-colonisation amongst children in day-care facilities, nurseries and kindergartens . Potential sources of C. difficile in the hospital setting include both symptomatic and asymptomatic patients and contaminated environments . Riggs et al.  suggested that asymptomatic patients contribute to CDI in long-term care facilities (LCFs), but it is uncertain whether intestinal carriage by healthy adults in the community acts as a reservoir and a potential source for community-associated CDI. Conversely, some authors suggested that asymptomatic carriage of C. difficile was associated with decreased risk of subsequent diarrhoea , while others believed that C. difficile was even not part of the normal faecal flora in elderly in-patients .
Carriage and transmission of C. difficile has been studied in the elderly living in LCFs , , as well as in healthy adults aged up to 65 years (median age 22 years) in Japan , , many of whom were University students. Reported asymptomatic carriage rates of the organism are contentious and vary up to 5-fold across several studies (4–20%) , –, in part due to differences in the population target, such as age, health and dwelling status, as well as the adoption of different culture and detection standards. To the best of our knowledge, there are no studies of carriage in healthy elderly individuals aged 65 years and over residing outside of LCFs. We have therefore studied the prevalence of asymptomatic faecal carriage of C. difficile in a healthy elderly cohort in the United Kingdom. Isolates were investigated to determine whether the strains isolated from these individuals were current endemic PCR-ribotypes and to assess their characteristics and distribution.
Materials and Methods
Ethics Statement: Ethical approval was obtained from the Liverpool Research Ethics Committee (ref. 08/H1005/32), and each participant volunteer gave written informed consent.
Two hundred and six members of a large, well studied longitudinal cohort of healthy elderly volunteers  residing in their own homes in different geographical areas in the north of England, mostly from Manchester and Newcastle metropolitan areas [Supporting Information – Figure S1], were approached and initially agreed to take part of a prospective study of CDI. All individuals were of white Caucasian origin and were enrolled as healthy age-matched controls with no clinical evidence of CDI.
A sample collection package was sent to participating volunteers with accompanying instructions. The package also contained a questionnaire which included questions about age, gender, a history of CDI in the preceding year and the details of any medication taken. Details of acid suppressive agents, including proton pump inhibitors, and antimicrobial therapy in the preceding four weeks were specifically requested. Volunteers were asked to return the stool sample and completed questionnaire by post to the Medical Microbiology Department in Liverpool. All samples were collected and received between August and September 2009.
Faecal samples were assessed according to the Bristol Stool Chart  and cultured for C. difficile by both direct and enrichment culture methods. Culture was performed with the faecal sample, either directly or after alcohol-shock treatment, on Brazier's cefoxitin-cycloserine egg yolk agar (CCEY, E & O Laboratories Ltd, Bonnybridge, UK) and then incubated for 48 h at 37°C in an anaerobic chamber. Similarly enrichment culture was performed by inoculating the faecal samples into the enrichment medium processed with and without alcohol-shock treatment . Cooked meat broth (Oxoid Ltd, Basingstoke, UK) supplemented (after autoclaving) with sodium taurocholate (0.05%, Alfa Aesar Ltd, Heysham, UK), lysozyme (5 mg/L, Sigma-Aldrich, Poole, UK), cycloserine (500 mg/L, Bioconnections, Wetherby, UK) and cefoxitin (16 mg/L, Bioconnections) was used as enrichment medium. All positive samples were tested using a second aliquot from the same submitted specimen to confirm initial results and multiple colonies selected for PCR-ribotyping. A faecal sample known to be culture and toxin positive for C. difficile (ToxA+, ToxB+) was used as a positive control and a broth inoculated with Escherichia coli ATCC 25922 was used as a negative control with each batch of specimens cultured. Samples in enrichment broth were incubated for 48 h at 37°C and then sub-cultured on to Brazier's CCEY agar and incubated anaerobically for 48 h at 37°C. Potential C. difficile isolates were identified by their characteristic smell and colonial morphology, fluorescence under long wave UV light and a latex agglutination test for C. difficile somatic antigen (Oxoid Ltd, Basingstoke, UK). Isolates were stored on PROTECT beads (Technical Services Consultants Ltd, Heywood, UK) at −70°C.
Faecal samples were tested for the presence of both C.difficile glutamate dehydrogenase (GDH) and toxins A and/or B using C. DIFF CHEK-60 and TOX A/B II ELISA immunoassay kits (Techlab, Blacksburg, USA), respectively. Briefly, approximate 100 µg of faeces was mixed with 400 µl of the provided diluent. The content was then vigorously shaken for 1 minute and centrifuged at 10,000 g for 1 minute. Supernatants were then collected and the immunoassay test carried out following the manufacturer's instructions. Plates were read at 450 nm and corrected at 540 nm wavelength.
Stored isolates were sub-cultured for toxin detection and PCR-ribotyping at a later date. A multiplex PCR assay targeting a species-specific internal fragment of the triose phosphate isomerase (tpi) housekeeping gene, internal core sequences of both toxins A (tcdA) and B (tcdB) genes was used to confirm all isolates as C. difficile and verify their individual toxigenicity . In addition, all isolates were tested for toxin expression. The isolate was inoculated into a 15 ml Brain Heart Infusion broth and cooked meat medium (Southern Group Laboratory Ltd, Corby, UK) and incubated anaerobically for 18–24 h at 37°C. Cultures were then centrifuged and the filtered supernatant used to test for the presence of toxins A and/or B using a TOX A/B II ELISA kit (Techlab, Blacksburg, USA). Isolates were typed by PCR-ribotyping according to the method described by Bidet et al  and compared to a panel of the commonest ribotypes circulating in the UK .
Faecal samples and questionnaires were received from 149 of the 206 volunteers approached; 23 declined consent while 34 did not respond. A summary of demographic information and faecal culture results is given in Table 1. All individuals in our study were aged over 70 years (median 81, IQR range, 72–90). The majority were female (79.9%), which reflects the higher enrolment rates by female volunteers as well as the presence of significant selective dropout since these volunteers are part of a large longitudinal cohort that has been monitored for more than 25 years .
Among the individuals recruited, only one reported having CDI in the previous 12 months; however this individual was not culture positive for C. difficile. Nine (6%) volunteers had a history of major gastrointestinal conditions, such as Crohn's disease, ulcerative colitis, colectomy/cecotomy and colostomy. At the time of assessment, 137 of our volunteers (91.9%) were taking medication. Thirty-one (21.4%) were taking acid suppressive agents, but only 16 (10.8%) had taken any form of antimicrobial in the four weeks before providing a sample [Table 1].
All 149 stool samples submitted were considered formed and none were liquid (type 6 or 7 according to the Bristol stool chart). One sample was positive for C. difficile by both direct culture and enrichment culture. Another sample was negative by direct culture but positive by enrichment culture of the faecal sample treated with and without alcohol-shock. A further four samples were positive only by the enrichment culture method without alcohol-shock treatment [Table 2]. Three isolates were toxigenic (ToxA+, ToxB+) and four were non-toxigenic (ToxA-, ToxB-) based on our in vitro assay. No faecal samples were directly positive for Toxin A and/or B by the ELISA test. Only one of the 149 faecal samples tested was positive by GDH ELISA; this sample was also positive by direct culture. The other five samples that were positive by the enrichment culture method were negative for GDH. Three of these 6 individuals (50%) with C. difficile carriage were taking acid-suppressive agents compared to 28/139 (20.1%) of those who were free of C. difficile (RR = 2.48 [95% CI 0.89–4.70], X2 = 1.53, p = 0.22). Conversely, none of these positive subjects had history of CDI in the past 12 months, and neither did they report use of any antimicrobials in the previous 3 months prior to the recruitment.
Four out of the seven strains identified in the volunteers were of non-toxigenic types based on toxin gene screening. PCR-ribotyping confirmed that the four non-toxigenic isolates had the following PCR-ribotypes: 009, 026 (n = 2) and 039. Two of them shared the same ribotype and one volunteer was found to concurrently carry two distinct strains: PCR-ribotypes 003 and 039 [Supporting Information - Figure S2], the former being toxigenic. This sample was positive on direct culture and was the single GDH positive faeces. Further samples were obtained from this volunteer and showed continued carriage of the strain type (PCR-ribotype 003) 12 months after the initial sample. No antibiotics or proton pump inhibitors were used during the one year follow-up. The other two toxigenic C. difficile strains observed in our cohort were PCR-ribotypes 005 and 106, which are amongst the most common strains circulating in the UK . On further questioning it emerged that the individual carrying PCR-ribotype 005 worked regularly as a volunteer in a hospital, where this strain was prevalent.
The strength of this study is that it evaluates the presence of C. difficile in healthy elderly individuals living in the community, from a very well documented cohort . All individuals were living in their own homes rather than in a nursing home care facility or in hospitals and we did not find evidence for geographical location clustering of positive volunteers. The overall carriage rate of 6/149 (4%) was considerably lower than that of a previous report by Brazier et al. , who found rates of 10.2% for carriage (47/284) and 6.3% (18/284) for eventual nosocomial acquisition amongst elderly patients admitted to 6 Welsh hospitals in 1999. In addition, two studies on healthy adults in Japan by Kato et al. in 2001  and Ozaki et al. in 2004  reported the presence of C. difficile in 94 of 1,234 subjects (7.6%) and 8 of 139 subjects (5.8%), respectively. The reported carriage rate with toxigenic strains were 4% in the two studies, compared with 2% in our study. An investigation conducted in long-term care facilities in the USA by Walker  found carriage rates of 7.1% in 225 subjects, whereas another American study  reported a rate of 5% (2 in 42 subjects) and a recent Irish investigation observed a prevalence of asymptomatic C. difficile carriage of 10 in 100 patients (10%), 7 of which were toxin positive (7%) . These rates are considerably lower than the carriage rate of 19% reported by Simor et al  in nursing home patients in Canada. It is important to note that, with exception of the latter study , all the above investigations have used standard direct culture methods only and their figures would have been higher had they used enrichment culture methods. The fact we have also identified a sample which produced two distinct strains also highlights the need for testing multiple colonies isolated from the same specimen in order to further validate results.
While the Toxin A/B Elisa kit did not identify any positive samples, only one of the 149 faecal samples tested was positive by the GDH ELISA test. This sample was also positive by direct culture and remained culture positive 12 months after the first sample collection. The other five samples that were positive by enrichment culture only were negative for GDH. Although GDH assays reportedly have high specificity to C.difficile , it is very likely that the levels of GDH antigen in these samples were below the lower detection threshold for this test. Our results suggest that the GDH assay is significantly less sensitive than enrichment culture methods and reinforces the importance of enrichment culture for the screening of solid or semi-solid stools from healthy volunteers.
We found a range of distinct PCR-ribotypes consistent with the concept that the population of C. difficile in the community is significantly more diverse than in LCFs. The fact that two of the most common toxigenic PCR-ribotypes in the UK (i.e. 005 and 106) were found in our elderly cohort is not surprising. A previous screening study in Welsh hospitals found that over 50% of the strains isolated from elderly patients on admission were of PCR-ribotype 001, which was the most common strain circulating in hospital settings in the UK at the time . Conversely, the endemic strain smz, the most frequent type isolated from CDI patients at that time and known to have caused multiple outbreaks in Japan, was not found in any healthy carriers by Kato et al. . The epidemic strain type 027/NAP1/BI, which has largely accounted for the recent upsurge in the number of CDI cases, and has predominated in hospital settings in the United Kingdom  and Europe was not detected in our community-based elderly population. Although it is widely acknowledged that the epidemic PCR-ribotype 027 possesses additional virulence factors, such as hyperproduction of toxins  and increased sporulation rate , , it remains unclear whether its carriage is less likely to be asymptomatic in the elderly. Riggs et al. proposed that asymptomatic carriers are a potential source for transmission of epidemic and non-epidemic strains among LCF residents . While this is likely to happen in a shared environment, it is uncertain whether carriage by healthy adults in the community is a potential source for community-associated CDI, particularly infections accounted by hypervirulent epidemic strain types, such as PCR-ribotype 027.
It is widely acknowledged that the diversity of C. difficile population is favoured by the absence of strong selective pressure, which is a process commonly triggered by antimicrobial agents. None of the six culture positive individuals gave a history of antimicrobial treatment in the past four weeks or hospital admission in the preceding 12 months. Three of the six positive individuals were receiving acid-suppressive agents. Although this trend is consistent with the suggestion that these agents facilitate colonisation by C. difficile –, our study was underpowered to demonstrate any statistically significant differences given the low frequency of culture positive samples observed in our cohort.
The frequency and distribution of gastrointestinal carriage of C.difficile varies across different population groups. Indeed, Kato et al. found that carriage rates varied across occupational groups, such as university students, hospital workers, employees of a company and defence force personnel . Age is another important predisposing factor. Asymptomatic carriage is higher in neonates and young infants than in adults, while at the same time, the distribution of symptomatic CDI cases is much more skewed towards the elderly. This suggests the existence of biological factors mediating initial colonisation and onset of the disease and highlights the importance of investigating both the symptomatic and asymptomatic carriage of C. difficile in the elderly. This study confirms that the carriage ratio of C. difficile amongst elderly individuals residing in their own homes in different geographical areas is likely to be lower than rates reported for individuals in LCFs, even after adopting enrichment methods to enhance the recovery of the organism. Hence, higher rates in LCFs probably reflect the greater probability of cross-contamination of the organism in these settings, as well as other contributing factors such as frailty, polypharmacy and increased use of medicines, such as proton pump inhibitors and antimicrobials.
Elderly individuals are a difficult group to recruit and one limitation of our study is the lack of follow-up to distinguish transient carriage from longer term colonisation. In a single individual we were able to conduct follow-up and demonstrated persistent carriage for one year. Another potential source of bias is the considerably higher rate of females in our cohort. This can partly be attributed to their greater longevity and to the lower enrolment and higher dropout rates among males of the original longitudinal study. The investigation of asymptomatic carriers in the community is important, not only to assess the host susceptibility to CDI, but also for the identification of novel pathogen factors associated with virulence and antimicrobial resistance. A clearer understanding is needed of why in some populations, such as neonates and children, C. difficile acts as a commensal but in others it becomes a pathogen. There is growing evidence that primary asymptomatic carriage of the organism may constitute a protective status against subsequent CDI by allowing the organism to mount an effective immune response. This, for example, constitutes the basis of recent vaccine trials for preventing recurrent CDI using multiple doses of non-toxigenic C.difficile strains as inducers . A prospective investigation of a cohort of symptom-free C. difficile carriers to ascertain who might develop symptomatic infection could also help address this question.
Geographic distribution of volunteers recruited by this study. A. British Isles; B. Close-up in the North of England.
PCR-Ribotyping results of the 7 strains recovered by both direct and enrichment methods. Note that sample 3 generated isolates of two distinct ribotypes. “No-Alcohol” indicates no alcohol-shock treatment prior to the culture; “Alcohol” indicates alcohol-shock treatment prior to the culture “Enrichment” denotes enrichment culture, “Direct” denotes direct culture.
We thank the recruits who kindly volunteered for this study. We are grateful to our colleagues from the University of Liverpool and the Royal Liverpool University Hospital for their valuable support, especially Vivien Plat for the help in assembling the collection kits, Mark Hopkins for some technical suggestions, Anita Hanson and Sarah Heslop for assisting with the ethics requirements of the project, Jack Waterson for the data entry and Drs. Godfrey Smith and James Anson for their clinical advice.
Ethics approval was obtained to conduct the study from the Liverpool Research Ethics Committee, ref. 08/H1005/32.
Conceived and designed the experiments: MP CP FM PHR NP MH. Performed the experiments: PHR FM AS VP JB. Analyzed the data: FM AS PHR. Contributed reagents/materials/analysis tools: MJ NP MH MP. Wrote the paper: FM PHR. Collection kits: FM AS. Facilitated recruitment: MJ NP MH. Clinical input: CP NP MH NB MP.
- 1. Kuijper EJ, Van Dissel JT, Wilcox MH (2007) Clostridium difficile: Changing epidemiology and new treatment options. Current Opinion in Infectious Diseases 20: 376–383.
- 2. Warny M, Pepin J, Fang A, Killgore G, Thompson A, et al. (2005) Toxin production by an emerging strain of Clostridium difficile associated with outbreaks of severe disease in North America and Europe. Lancet 366: 1079–1084.
- 3. Deneve C, Janoir C, Poilane I, Fantinato C, Collignon A (2009) New trends in Clostridium difficile virulence and pathogenesis. International Journal of Antimicrobial Agents 33:
- 4. Stabler RA, He M, Dawson L, Martin M, Valiente E, et al. (2009) Comparative genome and phenotypic analysis of Clostridium difficile 027 strains provides insight into the evolution of a hypervirulent bacterium. Genome Biol 10: R102. gb-2009-10-9-r102 [pii];10.1186/gb-2009-10-9-r102 [doi].
- 5. Dial S, Delaney JAC, Barkun AN, Suissa S (2005) Use of gastric acid-suppressive agents and the risk of community-acquired Clostridium difficile-associated disease. Journal of the American Medical Association 294: 2989–2995.
- 6. Donta ST, Myers MG (1982) Clostridium difficile toxin in asymptomatic neonates. Journal of Pediatrics 100: 431–434.
- 7. Matsuki S, Ozaki E, Shozu M, Inoue M, Shimizu S, et al. (2005) Colonization by Clostridium difficile of neonates in a hospital, and infants and children in three day-care facilities of Kanazawa, Japan. International Microbiology 8: 43–48.
- 8. Gerding DN, Olson MM, Peterson LR (1986) Clostridium difficile-associated diarrhea and colitis in adults. A prospective case-controlled epidemiologic study. Archives of Internal Medicine 146: 95–100.
- 9. Riggs MM, Sethi AK, Zabarsky TF, Eckstein EC, Jump RLP, et al. (2007) Asymptomatic carriers are a potential source for transmission of epidemic and nonepidemic Clostridium difficile strains among long-term care facility residents. Clinical Infectious Diseases 45: 992–998.
- 10. Shim JK, Johnson S, Samore MH, Bliss DZ, Gerding DN (1998) Primary symptomless colonisation by Clostridium difficile and decreased risk of subsequent diarrhoea. Lancet 351: 633–636.
- 11. Campbell RR, Beere D, Wilcock GK, Brown EM (1988) Clostridium difficile in acute and long-stay elderly patients. Age and Ageing 17: 333–336.
- 12. Walker KJ, Gilliland SS, Vance-Bryan K, Moody JA, Larsson AJ, et al. (1993) Clostridium difficile colonization in residents of long-term care facilities: Prevalence and risk factors. Journal of the American Geriatrics Society 41: 940–946.
- 13. Rivera EV, Woods S (2003) Prevalence of asymptomatic Clostridium difficile colonization in a nursing home population: A cross-sectional study. Journal of Gender-Specific Medicine 6: 27–30.
- 14. Kato H, Kita H, Karasawa T, Maegawa T, Koino Y, et al. (2001) Colonisation and transmission of Clostridium difficile in healthy individuals examined by PCR ribotyping and pulsed-field gel electrophoresis. J Med Microbiol 50: 720–727.
- 15. Ozaki E, Kato H, Kita H, Karasawa T, Maegawa T, et al. (2004) Clostridium difficile colonization in healthy adults: Transient colonization and correlation with enterococcal colonization. J Med Microbiol 53: 167–172.
- 16. Simor AE, Yake SL, Tsimidis K (1993) Infection due to Clostridium difficile among elderly residents of a long- term-care facility. Clinical Infectious Diseases 17: 672–678.
- 17. Brazier JS, Fitzgerald TC, Hosein I, Cefai C, Looker N, et al. (1999) Screening for carriage and nosocomial acquisition of Clostridium difficile by culture: A study of 284 admissions of elderly patients to six general hospitals in Wales . Journal of Hospital Infection 43: 317–319.
- 18. Kyne L, Warny M, Qamar A, Kelly CP (2000) Asymptomatic carriage of Clostridium difficile and serum levels of IgG antibody against toxin A. New England Journal of Medicine 342: 390–397.
- 19. Simor AE, Bradley SF, Strausbaugh LJ, Crossley K, Nicolle LE, et al. (2002) Clostridium difficile in long-term-care facilities for the elderly. Infection Control and Hospital Epidemiology 23: 696–703.
- 20. Ryan J, Murphy C, Twomey C, Paul Ross R, Rea MC, et al. (2010) Asymptomatic carriage of Clostridium difficile in an Irish continuing care institution for the elderly: Prevalence and characteristics. Irish Journal of Medical Science 179: 245–250.
- 21. Rabbitt PMA, McInnes L, Diggle P, Holland F, Bent N, et al. (2004) The University of Manchester longitudinal study of cognition in normal healthy old age, 1983 through 2003. Aging, Neuropsychology, and Cognition 11: 245–279.
- 22. Lewis SJ, Heaton KW (1997) Stool form scale as a useful guide to intestinal transit time. Scandinavian Journal of Gastroenterology 32: 920–924.
- 23. Brazier JS (1993) Role of the laboratory in investigations of Clostridium difficile diarrhoea. Clinical Infectious Diseases 16: S228–S233.
- 24. Lemee L, Dhalluin A, Testelin S, Mattrat MA, Maillard K, et al. (2004) Multiplex PCR targeting tpi (triose phosphate isomerase), tcdA (toxin A), and tcdB (toxin B) genes for toxigenic culture of Clostridium difficile. J Clin Microbiol 42: 5710–5714.
- 25. Bidet P, Barbut F, Lalande V, Burghoffer B, Petit JC (1999) Development of a new PCR-ribotyping method for Clostridium difficile based on ribosomal RNA gene sequencing. FEMS Microbiology Letters 175: 261–266.
- 26. Health Protection Agency (2009) pp. 1–19. Clostridium difficile Ribotyping Network for England and Northern Ireland 2008/09 Report.
- 27. Eastwood K, Else P, Charlett A, Wilcox M (2009) Comparison of nine commercially available Clostridium difficile toxin detection assays, a real-time PCR assay for C. difficile tcdB, and a glutamate dehydrogenase detection assay to cytotoxin testing and cytotoxigenic culture methods. J Clin Microbiol 47: 3211–3217.
- 28. Akerlund T, Persson I, Unemo M, Noren T, Svenungsson B, et al. (2008) Increased sporulation rate of epidemic Clostridium difficile type 027/NAP1. J Clin Microbiol 46: 1530–1533.
- 29. Merrigan M, Venugopal A, Mallozzi M, Roxas B, Viswanathan VK, et al. (2010) Human hypervirulent Clostridium difficile strains exhibit increased sporulation as well as robust toxin production. Journal of Bacteriology 192: 4904–4911.
- 30. Martinsen TC, Bergh K, Waldum HL (2005) Gastric juice: A barrier against infectious diseases. Basic and Clinical Pharmacology and Toxicology 96: 94–102.
- 31. Hookman P, Barkin JS (2009) Clostridium difficile associated infection, diarrhea and colitis. World Journal of Gastroenterology 15: 1554–1580.
- 32. Kaur S, Vaishnavi C, Prasad KK, Ray P, Kochhar R (2007) Comparative role of antibiotic and proton pump inhibitor in experimental Clostridium difficile infection in mice. Microbiology and Immunology 51: 1209–1214.
- 33. Tatarowicz W, Seiberling M, Gerding DN, Gomez A, Monnot-Chase E, et al. (2010) Safety and Tolerability of an oral suspension of VP 20621, spores of a non-toxigenic Clostridium difficile strain, in healthy older subjects. Abstract Book - 3rd International Clostridium difficile Symposium 44: