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We identified a predominant clone of Clostridium difficile PCR ribotype 002, which was associated with an increased sporulation frequency. In 2009, 3,528 stool samples from 2,440 patients were tested for toxigenic C. difficile in a healthcare region in Hong Kong. A total of 345 toxigenic strains from 307 (13.3%) patients were found. Ribotype 002 was the predominant ribotype, which constituted 35 samples from 29 (9.4%) patients. The mean sporulation frequency of ribotype 002 was 20.2%, which was significantly higher than that of the 56 randomly selected ribotypes other than 002 as concurrent controls (3.7%, p<0.001). Patients carrying toxigenic ribotype 002 were more frequently admitted from an elderly home (p=0.01) and received more β-lactam antibiotics in the preceding 3 months compared with the controls (p=0.04) . The identification of toxigenic ribotype 002 in 2009 was temporally related to a significant increase in both the incidence of toxigenic C. difficile from 0.53 to 0.95 per 1,000 admissions (p<0.001) and the rate of positive detection from 4.17% to 6.28% (p<0.001) between period 1 (2004–2008) and period 2 (2009). This finding should alert both the physician and the infection control team to the establishment of and possible outbreaks by ribotype 002 in our hospitals, as in the case of ribotype 027.
Clostridium difficile is an anaerobic, Gram-positive, spore-forming bacillus which causes gastrointestinal diseases ranging from antibiotic-associated diarrhea to pseudomembranous colitis. Though community-acquired infection can occur, most cases are found in the hospital and long-term care facilities . The fecal colonization rate in ambulatory individuals is up to 2% [2, 3] and this increased to 15–30% among hospitalized patients due to the acquisition from healthcare workers and the hospital environment . About 15–60% of the colonized patients develop symptomatic diarrhea during hospitalization [5–7], which may increase the nosocomial transmission of C. difficile with hospital outbreaks. Recently, a virulent strain identified as PCR ribotype 027, toxinotype III, or North American pulse-field type 1 has emerged to cause severe colitis, leading to a high mortality rate [8–10]. The mechanism of increased virulence is still under investigation, but it may be related to the 18-bp deletion and single-base-pair deletion at position 117 in the toxin regulator gene (tcdC), leading to the hyperproduction of toxins A and B [11, 12]. In addition, increased sporulation frequency of certain epidemic strains of C. difficile PCR ribotype 027 may also contribute to its better survival and nosocomial spread [13, 14]. Sporulation occurs when the ability to maintain vegetative growth has failed and facilitates the transmission of C. difficile in the healthcare setting, as the spores remain infective and persist in the environment for many months .
A sporadic case of C. difficile PCR ribotype 027 was reported in Hong Kong in 2008 . In response to this emerging infectious agent, further investigation was performed on all C. difficile isolates in a healthcare region in Hong Kong. We also conducted a retrospective review of the clinical and epidemiological data related to the different ribotypes of toxigenic C. difficile isolated in 2009. The findings and their potential implications in disease transmission and infection control practice are discussed.
A surveillance program was conducted in a regional microbiology laboratory in Hong Kong. The laboratory provided service to a healthcare network of five hospitals, including one acute care university teaching hospital with 1,400 beds and four chronic care hospitals with 110 to 524 beds. The hospital network provided clinical service to a population of approximately 0.53 million people. Between 1 January 2009 and 31 December 2009, stool specimens from hospitalized patients sent for culture and cytotoxin assay of C. difficile were performed by our routine service protocol as usual, but the toxigenic strains were further characterized by molecular tests. The incidence of toxigenic C. difficile per 1,000 admissions and the rate of detection identified between period 1 (2004 and 2008) and period 2 (2009) were analyzed using databases of the laboratory information and hospital record system.
Liquid or semisolid stool samples were tested within 24 h of receipt. The samples were inoculated onto cycloserine–cefoxitin–fructose agar (CCFA) containing 4% proteose peptone, 0.5% Na2HPO4, 0.1% KH2PO4, 0.01% MgSO4, 0.2% NaCl, 0.6% fructose, 1.5% agar at pH 7.4 (#CM0601, Oxoid, UK), with added selective supplement containing 250 mg/L D-cycloserine, 8 mg/mL cefoxitin (#SR0096, Oxoid, UK), and 7% horse blood. Culture plates were incubated anaerobically at 35°C to 37°C for 48 h. Obligatory anaerobic, large Gram-positive bacilli that were isolated from the CCFA and were susceptible to 5 μg of vancomycin were presumptively identified as C. difficile. The identification was confirmed by the Vitek® Anaerobe Identification Card (ANI) (bioMérieux, Inc., USA). Antimicrobial susceptibility testing against metronidazole, vancomycin, and ciprofloxacin were performed for selected strains using Etest strips according to the manufacturer’s instructions (AB Biodisk, Sweden).
Approximately 3 to 5 g of stool was suspended in 5 ml of phosphate-buffered saline (PBS) in a 1:2 dilution at a pH level of 7. The sample was centrifuged at 3,000 rpm for 55 min to produce a supernatant, which was subsequently transferred into eppendorf tubes and centrifuged at 13,000 rpm for 15 min at 4°C to clarify the supernatant. The supernatant was passed through a 0.22-μm-pore-size membrane filter. A toxin-producing C. difficile strain (UKEQAS QC 6109) was used as the positive control for the cell culture cytotoxicity neutralization assay (CCCNA), which was performed in sterile 96-well plates coated with the HeLa cell line as previously described . In addition to the direct detection of cytotoxin from stool filtrates, CCCNA was also performed on the stationary-phase culture supernatant of each C. difficile isolate. C. difficile isolates were subcultured to brain heart infusion broth and incubated anaerobically for 96 h. Culture supernatant was subjected to CCCNA as for stool filtrate with the same interpretation criteria as previously described .
DNA was extracted from C. difficile colonies using alkaline lysis as described previously . Polymerase chain reaction (PCR) ribotyping was performed according to the method described by Bidet et al. . After the electrophoresis of PCR products, the phylogenetic tree was constructed using BioNumerics v6.0 software (Applied Maths, Belgium).
slpA typing was performed for selected strains belonging to the same ribotype according to Joost et al. . The purified PCR product was subjected to cycle sequencing by ABI BigDye terminator v1.1 (Applied Biosystems, Foster City, USA) and the resulting slpA sequence was compared to those in the NCBI database by using Nucleotide BLAST.
The Miles and Misra method was adopted to study all PCR ribotype 002 isolates . C. difficile was subcultured to C. difficile agar (Mast Group Ltd., Merseyside, UK) and incubated at 37°C anaerobically for 72 h. Bacterial suspension was prepared in saline to a turbidity of McFarland standard 0.5, followed by serial dilutions in saline to 101–104. Twenty microliters of each bacterial suspension with dilutions from 102 to 104 were transferred to three sectors of 12 blood agar plates from a height of 2.5 cm. The inoculum was spread over an area of 1.5–2.0 cm diameter. One set of agar plates (six blood agar plates) were incubated for 72 h at 37°C anaerobically and the other set of agar plates (six blood agar plates) were incubated for 48 h at 37°C aerobically, followed by a further incubation of 72 h at 37°C anaerobically. The sporulation frequency (the spore/total cell ratio), expressed as a percentage, was determined by dividing the average cell count of the second set over the first set. To rule out cross-contamination by other Clostridium species in the experiment , PCR for C. perfringens and C. difficile was performed on bacterial suspensions and colonies according to previously described methods [22, 23].
Toxins A and B were measured by the C. difficile TOX A/B II™ kit (TechLab, the Netherlands), according to the manufacturer’s instructions. All strains belonging to the PCR ribotype 002 were subcultured into brain heart infusion broth and incubated for 72 h anaerobically. Bacterial suspension was centrifuged at 3,000×g for 10 min and 50 μl of supernatant was mixed with 200 μl of diluent supplied in the kit. One drop (50 μl) of conjugate was added to the well of a microassay plate with immobilized affinity-purified polyclonal goat antibody against toxins A and B. The 100 μl diluted sample was transferred and mixed with the conjugate in the wells. The plate was incubated at 37°C for 50 min, washed four times with 1X wash solution, followed by the addition of 100 μl substrate solution. Stop solution was added to terminate the reaction after 5 min of incubation at room temperature. The resulting yellow color change was quantified by measuring the optical density 450 nm/620 nm. An A450/620 value of 1.0 corresponded to 1 U of the total amount of toxins (A and B).
Patients with toxin-producing C. difficile were assessed by infection control nurses for symptomatology. Case records were reviewed if the patients had been discharged. Patients with diarrhea at the time of specimen collection were classified as having symptomatic infection, while those without diarrhea were classified as having asymptomatic colonization. Patients with symptomatic infection were further classified as having healthcare-associated infection, of which the development of symptoms started more than 48 h after admission to the hospital or within 4 weeks after discharge from the hospital, or community-associated infection, of which the development of symptoms started within 48 h after admission to the hospital or more than 12 weeks after discharge from the hospital, as previously described [24, 25]. When symptoms developed 4–12 weeks after hospital discharge, the association was indeterminate. The disease severity was stratified according to a scoring system described previously . Briefly, two points were given to patients with endoscopic confirmation of pseudomembranous colitis or those requiring intensive care support. One point each was given for age >60 years, temperature >38.3°C, albumin level <2.5 mg/dL, and peripheral WBC count >15,000 cells/mm3 within 48 h of symptom onset. Patients with two points or more were considered as having “severe C. difficile-associated diarrhea (CDAD)”. Otherwise, the patient was stratified as having “C. difficile infection”. The demographics of the patients with C. difficile ribotype 002 and 56 randomly selected patients with PCR ribotypes other than 002 were compared.
The toxin level of all strains of C. difficile PCR ribotype 002 were determined by ELISA. The sporulation frequency of C. difficile PCR ribotype 002 was measured by the quantitative method described above. The correlation between the sporulation frequency and toxin level was assessed. The sporulation frequencies and toxin levels of the strains isolated from patients with symptomatic infection were compared to those from asymptomatic patients. The sporulation frequency was tested in 56 randomly selected strains of PCR ribotypes other than 002 (one strain of 001, six strains of 012, three strains of 014, two strains of 017, eight strains of og39, and 36 strains of other patterns) as the control.
Fisher’s exact test and Student’s t-test were used in the analysis, where appropriate. Changes in the incidence of toxigenic C. difficile per 1,000 admissions between period 1 (2004–2008) and period 2 (2009) was analyzed by Poisson regression. Correlation between sporulation frequency and toxin level was assessed by Spearman’s rank correlation coefficient. All reported p-values were two-sided. A p-value of <0.05 was considered to be statistically significant. Computation was performed using the Statistical Package for the Social Sciences (SPSS) version 15.0 for Windows.
Between 1 January 2009 and 31 December 2009, a total of 3,528 stool samples from 2,440 patients were tested for C. difficile culture and cytotoxin assay. A total of 169 samples from 145 (5.9%) patients were found to have cytotoxin production by CCCNA from both stool filtrates and C. difficile isolates. Another 176 samples from 162 (6.6%) patients had negative cytotoxin production in stool filtrates but positive toxin production in the culture supernatant of C. difficile isolates (Fig. 1). A total of 345 toxigenic C. difficile strains from 307 (12.5%) patients were further tested for ribotyping and the results are listed in Table 1. All PCR ribotypes concurred with slpA typing results. PCR ribotype 002 was the most predominant ribotype, constituting 35 strains from 29 (9.4%) patients with toxin-producing C. difficile. The dendrogram of C. difficile PCR ribotype 002 is shown in Fig. 2. All 35 strains of PCR ribotype 002 were resistant to ciprofloxacin (minimum inhibitory concentration [MIC]>32 μg/ml). The MIC50 of metronidazole and vancomycin were 0.5 μg/ml and 0.75 μg/ml, respectively, whereas the MIC90 were 0.75 μg/ml and 1.5 μg/ml, respectively. The change in incidence of toxigenic C. difficile per 1,000 admissions and the rate of positive detection in our healthcare region from 2004 to 2009 are shown in Fig. 3. There was a significant increase in both the incidence of toxigenic C. difficile from 0.53 to 0.95 per 1,000 admissions (p<0.001) and the rate of positive detection from 4.17% to 6.28% (p<0.001) between period 1 (2004–2008) and period 2 (2009).
During the study period, a total of 29 patients shed C. difficile ribotype 002 in the stool. There were 20 males and 9 females, with a median age of 76 years (range 14–97 years). Eleven (37.9%) patients were old age persons home residents. Symptomatic infection was diagnosed in 17 (58.6%) patients, while ten of them had severe CDAD according to the scoring system (Table 2). All 17 patients with symptomatic infection were defined as healthcare-associated infection. Colonization of C. difficile was found in 12 (41.4%) patients. Most of the patients (24, 82.8%) were managed in the medical ward, while three patients were managed in the surgical ward, one patient in the emergency department, and one patient in the pediatric and adolescent unit. These patients were located in 20 different wards from three different hospitals (one acute care and two chronic care hospitals) without any epidemiological linkage. There were five patients with repeated isolation of C. difficile during the same episode of hospitalization, among whom four patients had two episodes and one patient had three episodes. Among these five patients, three had symptomatic infection and one had asymptomatic colonization. The other progressed from asymptomatic colonization to symptomatic infection during hospitalization. The demographic characteristics of patients with C. difficile PCR ribotype 002 and ribotypes other than 002 are illustrated in Table 3. Patients carrying toxigenic C. difficile PCR ribotype 002 were more frequently admitted from an elderly home (p=0.01) and received more β-lactam antibiotics in the preceding 3 months (p=0.04).
There is no statistically significant correlation between the sporulation frequency and the measured toxin levels of the C. difficile isolates (Spearman’s rho 0.0311, p=0.858). The mean sporulation frequency of 35 strains of C. difficile PCR ribotype 002 was 20.2%, which was significantly higher than that of the 56 randomly selected PCR ribotypes other than 002 (3.7%, p<0.001). Among the 23 strains of C. difficile PCR ribotype 002 isolated from patients with symptomatic infection, the mean sporulation frequency was significantly higher than 12 strains of PCR ribotype 002 cultured from patients with asymptomatic colonization (28.9% vs. 3.5%, p=0.02). The mean levels of toxin production by ELISA among strains collected from patients with asymptomatic colonization and symptomatic infection were 96.13 U/ml and 123.85 U/ml, respectively (p=0.29). Subgroup analysis for the C. difficile isolated from symptomatic patients with or without severe CDAD showed no statistically significant difference in terms of sporulation frequency and toxin production.
C. difficile has become a re-emerging pathogen since the outbreak of a hypertoxigenic strain of PCR ribotype 027 in North America and Europe since 2003 [8, 10, 11]. This was followed by its global dissemination to the other continents in 2008 . On the other hand, C. difficile PCR ribotypes other than 027 have also been increasingly reported recently. PCR ribotype 078 has been implicated in community-associated C. difficile infection in the Netherlands , while PCR ribotypes 001 and 018 were the most commonly identified ribotypes in the healthcare facilities in Germany, the UK, and Italy [28–30]. Although C. difficile ribotype 027 has also been reported in Hong Kong in 2008 , our present study showed that PCR ribotype 002 was the most predominant strain and constituted 56% (35 out of 63 typed strains with well-characterized PCR ribotyping) of the C. difficile strains isolated in 2009. This finding might explain the significant increase in the positive detection rate of toxigenic C. difficile and the incidence of toxigenic C. difficile per 1,000 admissions observed in 2009 as compared to the baseline data between 2004 and 2008.
C. difficile PCR ribotype 002 was commonly found in patients with both symptomatic infection and asymptomatic colonization. The mean sporulation frequency (20%) of our strains was significantly higher than the other PCR ribotypes in our locality, but was comparable to that of the epidemic strains of C. difficile PCR ribotype 027 . Since the epidemic strains of C. difficile were reported to have an inherently increased sporulation frequency [13, 31], and the transmission of C. difficile in the healthcare facilities was mediated primarily by spores found in the environment or carried by healthcare workers [32, 33], C. difficile PCR ribotype 002 might, thus, become an epidemic strain and contribute to hospital outbreaks. In fact, all 17 symptomatic patients carrying PCR ribotype 002 had healthcare-associated C. difficile infection. Furthermore, as the proportion of patients residing in elderly homes was significantly higher among those with PCR ribotype 002 than those with other ribotypes, further investigations should be conducted in order to determine whether elderly homes might serve as an epidemic center amplifying this particular ribotype in our locality.
Interestingly, C. difficile PCR ribotype 002 isolated from patients with symptomatic infection had a significantly higher rate of sporulation, but not to the level of toxin production in vitro. Furthermore, there was no correlation between toxin production and sporulation. Our finding was in concordance with a recent study which suggested toxin production and sporulation to be opposite survival strategies for C. difficile in response to nutrient limitation by demonstrating an inverse correlation between toxin level and spore count in stationary-phase cultures . However, a more recent analysis of a hypervirulent strain of C. difficile exhibited an increased sporulation as well as toxin production . Since sporulation and toxin production is a complex process , and the disease severity of C. difficile is also determined by host factors such as the age, underlying diseases, and levels of toxin-neutralizing antibodies [36, 37], the relationship between sporulation frequency and disease severity remains to be elucidated.
The emergence of C. difficile with an inherently increased sporulation such as PCR ribotypes 027, 001, and 002 poses a great challenge to the infection control team. There is increasing evidence that the use of fluoroquinolones is a major risk factor for CDAD in the hospital and long-term care facilities [38–42]. Similar to the other emerging PCR ribotypes of C. difficile, all of our ribotype 002 strains were resistant to fluoroquinolones with an MIC>32 μg/ml against ciprofloxacin. Since the use of fluoroquinolones is increasing globally and locally [43, 44], our antimicrobial stewardship program should no longer target broad-spectrum antimicrobial agents only and should extend to include fluoroquinolones as well [45, 46]. Of note, patients carrying C. difficile PCR ribotype 002 were more frequently found to have used β-lactam antibiotics, including penicillin, cephalosporin, and carbapenem, in the preceding 3 months to our analysis (Table 3). As most of the β-lactams have a relatively lower MIC against C. difficile [47–49], strains with inherently increased sporulation, such as PCR ribotype 002, may survive better than poorly sporulating ribotypes, despite β-lactam antibiotics therapy. The waterless alcohol-based hand rub, which has been highly advocated in the healthcare setting for hand hygiene, was not effective against the spores of C. difficile in the hands [50, 51], even with directly observed hand hygiene practice . Therefore, a timely laboratory diagnosis to recognize this high-risk strain would facilitate strategic infection control interventions, which should include the early identification of symptomatic cases for contact precautions with single-room isolation and thorough environmental cleaning with chlorine-based germicides in order to inactivate C. difficile spores. In fact, the use of non-chlorine-based cleaning agents has been associated with a paradoxical increase in sporulation, which may further enhance the nosocomial transmission of C. difficile [31, 53]. A close collaboration between the microbiology laboratory and the infection control team is essential for the successful prevention of nosocomial outbreaks of C. difficile PCR ribotype 002 in our healthcare region.
There were several limitations to this study. Firstly, as there was no standardized guideline on when to order stool testing for C. difficile in our hospital, the population of our samples may have been biased. This might contribute to the apparently higher proportion of asymptomatic colonization of ribotype 002 among our population than that previously reported for C. difficile in general [2–4]. However, the exact asymptomatic colonization rate of ribotype 002 has not been clearly documented elsewhere. Secondly, we only had 23 (20%) out of 116 control strains available for the full panel of PCR ribotyping . There might be a possibility of missing some important PCR ribotypes in our series. However, among 221 patients with unrecognized PCR ribotypes, there were 106 distinct patterns and no major cluster. Thirdly, we could not retrieve the archived strain from the early period and, thus, the origin of this C. difficile PCR ribotype 002 could not be ascertained. From the epidemiological perspective, the incidence of toxigenic C. difficile remained static (0.53 per 1,000 admissions) between 2004 and 2008, but it suddenly increased to 0.95 per 1,000 admissions in 2009. Although the incidence was lower than some centers in Europe and was still within an acceptable limit of less than 5 cases per 1,000 admissions as recommended by some experts [55, 56], an 80% upsurge should alert both the physician and the infection control team to possible outbreaks of ribotype 002 before it could become established in our hospitals, as in the case of C. difficile PCR ribotype 027.
We thank Dr. E.J. Kuijper (Leiden University, the Netherlands) for providing us the standard strains of C. difficile PCR ribotypes used as the positive control. The work was supported by the Research Fund for the Control of Infectious Diseases (RFCID) of the Food and Health Bureau (FHB) of the Hong Kong SAR Government.
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