Antimicrobial resistance in commensal flora of pig farmers.
Higher prevalence of antimicrobial-resistant bacteria in commensal flora contributes to the general increase and dissemination of bacterial resistance worldwide (1,2) and can be a source of resistance genes for respiratory pathogens such as Streptococcus pneumoniae (3) and intestinal pathogens such as Shigella (4) or Salmonella (5,6). Antimicrobial treatments are major factors for selection of resistance in the commensal flora of humans (7). Industrial animal farming is also associated with large-scale antimicrobial use (8), which leads to a high level of colonization of animals with antimicrobial-resistant bacteria that can then contaminate the food and, in turn, humans (9,10). Farmers are more likely to acquire enteric antimicrobial-resistant bacteria from food-producing animals, even if not treated with antimicrobial agents themselves (11-14). However, this link has never been quantitatively assessed. Antimicrobial resistance in nasal and pharyngeal commensal strains might possibly be affected in the same manner, and this hypothesis has also not been investigated. We thus designed an exposed-nonexposed epidemiologic study to determine the association between contact with animals in pig-raising farms and isolation of antimicrobial-resistant nasal, pharyngeal, and intestinal commensal microorganisms.
The study population was composed of members of the Mutualite Sociale Agricole (MSA), a health insurance system for workers in agriculture and related services. We identified pig farmers as an exposed group and nonfarmers (such as those working at banks or in insurance services) as a nonexposed group. The sample size was calculated according to results on the prevalence of antimicrobial resistance in the fecal flora of French residents (15) to ensure that, for most markers measured, detection of a 10% difference in the exposed group would be found with a power of 80% and an [alpha] risk of 5%. Pig farmers were chosen among those working in large, exclusively pig farms (>84 pigs) and contacted during the yearly MSA preventive medicine visits to obtain permission for participation. One pig farmer per farm was randomly selected to fill a panel of 20 in each of the seven major French porcine production areas.
One nonfarmer control, matched for sex, age, and county of residence, was selected for each pig farmer and approached similarly. Nonfarmers were not living or working on a farm, in a slaughterhouse, or in the pharmaceutical industry and were not living with someone who worked on a farm.
Persons included in the study were judged healthy by physical examination, had no gastrointestinal symptoms or throat pain at inclusion, and reported that they had not been hospitalized or taken antimicrobial agents within the previous month. All study participants were enrolled within 3 months. Study participants' antimicrobial use in the 6 months preceding the study was retrospectively estimated from the MSA reimbursement database and converted to defined daily doses, as described (16). In cases in which methicillin-resistant Staphylococcus aureus (MRSA) was isolated, participants were further interviewed for hospitalization and contacts with hospitalized patients and healthcare workers during the previous year, as described (17). Occurrence and type of contact with pigs and contact precautions used in farms were documented in pig farmers with a standardized questionnaire. This study was performed in agreement with legal and ethical French regulatory procedures.
Study participants were asked to bring fresh stool samples in sterile, closed cups. A sterile cotton swab was immersed in the sample. No procedure was implemented to ensure that participants brought their own stool specimens. They likely did, however, since participants were contacted during the yearly MSA preventive medicine visits by the practitioner with whom they had an established confidential relationship. Nasal swabs were inserted (1 cm) successively in both nares and rotated three times for 10 to 15 s. Pharyngeal samples were obtained by firmly pressing a swab over the tonsils and the posterior pharyngeal wall, and avoiding touching the jaws, teeth, or gingival when withdrawing the swab. All swabs were extemporaneously squeezed in sterile brain-heart infusion broth (BioMerieux, Marcy-l'Etoile, France) with 10% glycerol, immerged in liquid nitrogen within 6 hours, and stored at -80[degrees]C until processing.
Detection of Microbial Isolates
One hundred microliter--aliquots of all broth samples were plated as follows. For nasal samples, isolation of S. aureus was performed on Chapman agar (BioMerieux). Antimicrobial susceptibility of one isolate per participant was determined by using the disk diffusion technique (18).
For the pharyngeal samples, isolation of Streptococcus pneumoniae and [beta]-hemolytic streptococci was performed on 5% sheep blood Columbia agar; isolation of Haemophilus influenzae was performed on chocolate agar, Staphylococcus aureus on Chapman agar, and yeast on Chromagar (all BioMerieux). Isolation of antimicrobial-resistant nongroupable streptococci was performed on 5% sheep blood Columbia agar supplemented with nalidixic acid and colistin. Antimicrobial-resistant nongroupable streptococci were detected on the same medium, supplemented with ampicillin (4 mg/L) or erythromycin (1 mg/L). For feces, aliquots were plated on Chromagar, Cetrimide (Bio-Merieux), and Chapman agar for detection of yeasts, Pseudomonas aeruginosa, and S. aureus, respectively. Detection of enterococci of any resistance phenotype and of those resistant to erythromycin was performed on Bile-Esculin-agar (BEA) (BioMerieux) free of antimicrobial agents or supplemented with 5 mg erythromycin/L, respectively. Detection of vancomycin-resistant enterococci (VRE) was performed on BEA supplemented with 10 mg vancomycin/L after an enrichment step of 18 hours in broth containing 1 mg vancomycin/L, as described (19,20). The mechanism of vancomycin resistance was determined by polymerase chain reaction analysis, as described (21). Carriage of resistant enterobacteria was detected by using two separate procedures, as described (22), with modifications. In the first, designed to explore the subdominant flora, 0.1 mL of broth was plated on Drigalski agar supplemented with ampicillin (10 mg/L), ceftazidime (2 mg/L), streptomycin (20 mg/L), kanamycin (20 rag/L), chloramphenicol (20 mg/L), tetracycline (10 mg/L), or nalidixic acid (50 mg/L), as described (15). Escherichia coli of known susceptibility were used as the control. One of 10 positive plates was selected for quality control, and one colony was selected for antimicrobial susceptibility testing. A study participant was defined as colonized in the subdominant fecal flora with enterobacteria resistant to a given antimicrobial agent when at least one colony grew from the plate containing the corresponding antimicrobial agent.
In the second procedure, designed to explore the predominant fecal flora, Drigalski agar plates without antimicrobial agents were spread with 0.1 mL of broth culture. Five colonies were randomly selected. Those identified as E. coli were tested for antimicrobial susceptibility. A study participant was defined as colonized in the predominant flora by E. coli resistant to a given antimicrobial agent when at least one resistant strain was recovered from the feces by using this second procedure.
The prescribed defined daily doses of an antimicrobial agent and the number of participants for whom antimicrobial agents had been ordered within the previous 6 months were compared between pig farmers and nonfarmers by using the Student t test for matched data. Differences between groups for carriage of nasal, pharyngeal, and fecal microbial species were analyzed by calculating matched prevalence ratios (PR) (23). For comparing antimicrobial-resistant phenotypes of S. aureus, nongroupable streptococci, E. coli, enterococci, and enterobacteria from pig farmers and nonfarmer carriers, nonmatched PR were used, since these comparisons were performed on subgroups composed of only the carriers of the species with resistant clones that we examined. (For instance, rates of carriage of resistant enterobacteria were composed from subgroups of those actually carrying enterobacteria.) Because this analysis was performed only for carriers, a comparison in terms of age, sex, and location was performed to assess that pig farmers and nonfarmer carrier subgroups were comparable for these variables. Frequency of co-resistance to ampicillin, streptomycin, and trimethoprim-sulfamethoxazole in predominant strains of E. coli was used as a marker for multiple resistance and compared between groups (23). In analyzing data, we did not adjust for making multiple comparisons (24) since adjusting remains controversial (25,26), particularly for actual observations on nature (27). The association between isolation of resistant strains and specific farming activities and the size of farms was assessed by chi-square analysis.
We matched 113 exposed pig farmers with 113 nonexposed nonfarmers. The overall male-to-female ratio was 6.1, and mean age was 37.8 years (range 21 72). Mean previous time in the professional position occupied at the time of the study was 9.7 [+ or -] 1.9 and 13.0 [+ or -] 1.6 years for pig farmers and nonfarmers, respectively (p < 0.01).
Health insurance reimbursement data showed that antimicrobial agents had been prescribed in the month preceding the study for two pig farmers (one with macrolide and one with broad-spectrum penicillin 24 and 28 days before participation, respectively) and three nonfarmers (one with oral cephalosporin, one with penicillinase-resistant penicillin, and one with tetracycline 3, 10, and 24 days before participation, respectively). However, because of the retrospective nature of this analysis, the low number of participants, the nearly even distribution between pig farmers and nonfarmers, and the fact that reimbursement data are not a formal proof that antimicrobial agents were actually taken, these five persons were included in further analysis. Neither overall, nor class-specific antimicrobial prescriptions during the 6 months preceding participation in the study were significantly different between pig farmers and nonfarmers (Table 1). Prevalence of nasal or pharyngeal isolation of S. aureus was significantly higher in pig farmers (PR 1.85; confidence intervals [CI] 1.26 to 2.71]; p < 0.01) (Table 2). Isolation of erythromycin-resistant strains was significantly more frequent among S. aureus pig farmer carriers than among nonfarmer carriers (PR 9.72; CI 2.53 to 37.30; p < 0.01). Moreover, 31 (87%) of 36 macrolide-resistant S. aureus isolates from pig farmers were cross-resistant to lincosamides. Five pig farmers, but no nonfarmers, had MRSA (not significant). Analysis of the antimicrobial-susceptibility profile of these strains showed that two were resistant to at least one macrolide antimicrobial agent, four were resistant to aminoglycosides, and four were resistant to pefloxacin. Three of the MRSA carriers had been hospitalized within the 2 years preceding the study, including one within the previous year. The two other farmers had not been hospitalized but had visited outpatient clinics for medical problems within the year preceding the study.
Prevalence of pharyngeal isolation of Streptococcus pneumoniae, H. influenzae, and [beta]-hemolytic streptococci was low and did not differ significantly between groups (Table 3). One pig farmer carried yeast (Candida albicans). Isolation of nongroupable streptococci was frequent and not significantly different between groups, but that of nongroupable streptococci resistant to ampicillin was significantly more frequent in pig farmers than in nonfarmers (PR 2.02; CI 1.32 to 3.09; p < 0.01). Prevalence of fecal enterococci was not significantly different between groups nor was isolation of enterococci resistant to erythromycin or vancomycin (Table 4). In all, 16 VRE were isolated including 2 VanA-type Enterococcus faecium, along with 11 E. gallinarum and 3 E. casseliflavus of Vane phenotype and genotype. Nearly all participants carried enterobacteria: 103 (94.5%) of 109 pig farmers and 100 (91.7%) of 109 nonfarmers (PR 1.03; CI 0.96 to 1.10; not significant). Isolation of enterobacteria resistant to nalidixic acid (PR 7.12; CI 2.20 to 23.0; p < 0.01), chloramphenicol (PR 2.08; CI 1.17 to 3.68); p < 0.01), tetracycline (PR 1.65; CI 1.27 to 2.13; p < 0.01), and streptomycin (PR 1.40; CI 1.01 to 1.95; p < 0.01) was significantly more frequent in pig farmer carriers of enterobacteria than in nonfarmer carriers. Regarding the predominant flora, the most frequent species isolated were Escherichia coli (917/995; 92.2%) followed by Hafnia alvei (48/995; 4.8%) and Citrobacter freundii (11/995; 1.1%) with no significant between-group differences. The prevalence of isolation of E. coli resistant to cotrimoxazole (PR 3.02; CI 1.68 to 5.44; p < 0.01), tetracycline (PR 2.22; CI 1.48 to 3.32; p < 0.01), streptomycin (PR 1.40; CI 1.01 to 1.95; p - 0.04), or nalidixic acid (PR not calculable; p < 0.01) was significantly higher in pig farmers carrying E. coli than in nonfarmers (Table 4). In all instances in which subgroups of pig farmers and nonfarmers were compared, no significant between-group difference emerged in terms of age, sex, and county of residence. Prevalence of co-resistance to ampicillin, streptomycin, and cotrimoxazole was also significantly higher in E. coli from pig farmers (24%, 24/100) than from nonfarmers (12.2%, 12/98) (PR 1.96; CI 1.04 to 3.70; p = 0.03). No strains resistant to ceftazidime were isolated. No strains of Clostridium difficile, Pseudomonas aeruginosa, or Staphylococcus aureus were isolated from the feces of any study participant. Prevalence of yeast was not significantly different between pig farmers and nonfarmers, and the species were evenly distributed (Table 4).
Most pig farmers had several professional activities. Only a few farmers used isolation precautions (Table 5). We found no statistical association between professional activity or use of masks and gloves and the prevalence of resistant bacteria. By contrast, prevalence of nasal isolation of S. aureus resistant to macrolides increased significantly, from 33% (5/15) in pig farmers working in farms raising 84-180 swine, to 70% (7/10), 92% (11/12), and 100% (13/13) in those working in farms raising 181-270, 271-399, and >400 swine, respectively (chi-square linear slope; p < 0.01).
Our results showed that the prevalence of antimicrobial drug resistance in bacteria from the nasal, pharyngeal, and fecal flora was higher in pig farmers than in nonfarmers. With a few exceptions, pig farmers and nonfarmers had not taken antimicrobial agents during the month preceding the study and had not been differentially exposed to such agents during the previous 6 months. That E. coli (11-13) and enterococci (14) are significantly more resistant in persons working in farms or slaughterhouses than in urban residents had been reported, but a potential role of antimicrobial treatments in these workers could not be excluded and the increased prevalence of carriage of resistant organisms had not been quantified.
The prevalence of S. aureus nasal carriage in nonfarmers was similar to that reported previously in the general population (28), which suggests that the higher isolation rate in pig farmers was due to their work environment. This hypothesis was further supported by the increased resistance to macrolides (still the fourth most common class of antimicrobial agents used in food production ) of S. aureus isolates from pig farmers and the link between this resistance and the size of the farm. Why the isolation rate of S. aureus was higher in pig farmers remains unclear. Several hypotheses, including high transfer of animal specific clones, should be raised and investigated.
In the pharynx, ampicillin resistance of nongroupable streptococci in pig farmers may contribute to further transfer of [beta]-lactam resistance to Streptococcus pneumoniae by transformation (29). In the feces, antimicrobial drug resistance in enterobacteria was also greater in pig farmers for four of eight markers tested in the subdominant flora, and for four of nine markers in the predominant flora. Resistance in E. coli was close to that of healthy participants from developing countries (22). The prevalence of resistance in enterobacteria from the subdominant flora of our nonfarmers was lower than that in participants of the only study published that used the same methods; however, that study included mostly laboratory workers (A. Andremont, pers. comm.), who are known to be more colonized by resistant enterobacteria than are urban and rural dwellers (30). The rate of VRE colonization that we observed differed from that reported in France (31), which might be due to the enrichment step we used; however, the rate of VRE colonization did not differ between farmers and nonfarmers. This finding suggests that the 1997 ban (32) of avoparcin, a glycopeptide previously used as a growth promoter, was effective. Although specific information on avoparcin is lacking, 145 tons of antimicrobial agents were used globally in France in 1998 in pig raising, including 70 mg of growth additive per kilogram of pork meat produced (33).
Three possible explanations may explain why isolation of resistant bacteria in pig farmers was higher than in nonfarmers. First, farmers may come in contact with more antimicrobial-resistant bacteria from pigs; these bacteria are then transferred to the farmers. Second, farmers may be in frequent contact with antimicrobial agents themselves or antimicrobial residues that are given to the pigs in the workplace. The third possibility is that farmers receive more antimicrobial agents for other, i.e., medical, reasons. The first of these possibilities appears most likely because 1) farmers used very few precautions during contact with animal feces, 2) antimicrobial exposure is a well-known risk factor for intestinal yeast colonization (34,35), and yeast colonization in both groups was low, and 3) antimicrobial prescriptions were not significantly different between pig farmers and nonfarmers during the previous 6 months.
We did not assess the use of antimicrobial agents for animals in each of the 113 farms where pig farmers worked. However, 1,364 tons of antimicrobial agents were sold in France in 1999 for veterinary medicinal use. Of these, tetracycline, cotrimoxazole, and [beta]-lactams together accounted for 79.5% (8), a finding compatible with the high resistance rates found in pig farmers. However, we could not assess the exact cause of the high antimicrobial resistance rates in farmers. Determining the exact cause may not be as important as the fact that these people are colonized with a much higher rate of resistant bacteria. Further studies will need to be undertaken to identify the cause of this phenomenon.
Food products are a source of resistant bacteria (9,10). We minimized the risk that differences in food intake caused the higher prevalence of resistance in pig farmers by matching pig farmers with nonfarmers by age, sex, and county of residence. Children can be a source of resistant bacteria in households (36) and thus might be a confounding factor if the number of children was greater in pig farmer families than in nonfarmer families. However, this factor was not documented in the study questionnaire and thus could not be investigated.
Some inherent limitations of cross-sectional studies invite cautious assessments of our results. The lack of pre-exposure data on resistance and the general design of the study preclude determining a causal relationship between exposure and acquired resistance. However, the observation we made indicates that professional pig farming is significantly associated with isolation of antimicrobial-resistant commensal species. The minimal use of contact precautions by pig farmers may have further increased this risk, but the study was not designed to assess the efficacy of contact precautions, and thus no recommendations can be drawn in this matter.
Pigs could be raised with considerably fewer antimicrobial agents than currently used, and many animals can be raised with little or no exposure to such drugs at all (37). However, antimicrobial agents will still be used to treat sick animals. Additional studies are needed to evaluate the consequences of isolating resistant bacteria in farmers and, if necessary, design appropriate preventive measures.
Table 1. Total defined daily doses (DDD) of various classes of antimicrobial agents during the 6 months preceding participation in study (a) Total DDD (no. participants (b)) Antimicrobial agent Pig farmers Nonfarmers Penicillins (narrow-spectrum, 138 (9) 132 (9) broad-spectrum, and penicillinase-resistant) Cephalosporins 53 (7) 83 (9) Macrolides and lincosamides 67 (9) 35 (6) Others 15 (3) 67 (2) Total 273 (25) (c) 317 (19) (c) (a) As determined by health insurance reimbursements to pig farmers and nonfarmers. (b) Who used any given type of antimicrobial agent. (c) Some persons had multiple treatments. Table 2. Nasopharyngeal isolation of Staphylococcus aureus with various susceptibility to antimicrobial agents in pig farmers and nonfarmers (a) Prevalence no. (%) Type of S. aureus Pig farmers Nonfarmers Any 50/112 (44.6) 27/122 (24.1) Resistant to Methicillin 5 (b)/50 (10.0) 0/27 Macrolides 36/50 (72.0) 2/27 (7.4) Gentamicin 10/50 (20.0) 0/27 Pefloxacin 8/50 (16.0) 1/27 (3.7) Type of S. aureus Prevalence ratio 95% CI p value Any 1.85 1.26 to 2.71 <0.01 Resistant to Methicillin NA (c) 0.59 Macrolides 9.72 2.53 to 37.30 <0.01 Gentamicin NA NA 0.11 Pefloxacin 4.32 0.57 to 32.75 0.22 (a) Matched nasal samples were available for 112 pig farmer--nonfarmer pairs only. (b) In addition to being resistant to methicillin, two strains were resistant to at least one macrolide antibiotic (two were resistant [R] to erythromycin, lincomycin, and pristinamycin; 1 susceptible [S] to erythromycin only; and one susceptible to pristinamycin only), 4 strains were R to aminoglycosides (2 were RRS and 2 RRR to kanamycin, tobramycin, and gentamicin, respectively). Four strains were resistant to pefloxacin. (c) NA, not applicable. Table 3. Pharyngeal isolation of selected microorganisms in pig farmers and nonfarmers (a), (b) Prevalence, no. (%) Microorganisms Pig farmers Nonfarmers Streptococcus pneumoniae 0/112 (0) 3/112 (2.7) Haemophilus influenzae 6/112 (5.4) 5/112 (4.5) Enterobacteria 1/112 (0.9) 2/112 (1.8) Yeasts (c) 1/112 (0.9) 0/112 [beta]-hemolytic 11 (e)/112 (89.8) 9 (f)/112 (8.0) streptococci (d) NGS (g) Any 108/112 (6.4) 100/112 (89.3) Resistant to Ampicillin 48/108 (44.4) 22/100 (22.0) Macrolides 108/108 (100.0) 100/100 (100.0) Microorganisms Prevalence ratio 95% CI p value Streptococcus pneumoniae NA NA 0.25 Haemophilus influenzae 1.20 0.38 to 3.82 1.00 Enterobacteria 0.50 0.05 to 5.44 1.00 Yeasts (c) NA NA 0.25 [beta]-hemolytic 1.22 0.53 to 2.83 0.82 streptococci (d) NGS (g) Any 1.08 1.00 to 1.16 0.06 Resistant to Ampicillin 2.02 1.32 to 3.09 <0.01 Macrolides NA NA 1.00 (a) Matched pharyngeal samples were available for 112 pig farmer-nonfarmer pairs. (b) CI, confidence interval; NA, not applicable. (c) Candida albicans. (d) Several species were present in some study participants. (e) Group A strcptococcus: 1, group C: 5, S. anginosus: 3, S. intermedius: 1, S. constellatus: 4. (f) Group A streptococcus: 1, group C: 5, S. anginosus: 3, S. intermedius: 1, S. constellatus: 3. (g) Nongroupable streptococci. Table 4. Fecal isolation of selected microorganisms in pig farmers and in nonfarmers Prevalence no. (%) Microorganisms Pig farmers Nonfarmers Enterococci Any 71/109 (65.1) 80/109 (73.4) Resistant to Erythromycin 38/71 (53.5) 46/80 (57.5) Vancomycin 6 (b)/71 (8.5) 10 (c)/80 (12.5) Enterobacteria (d) Any 103/109 (94.5) 100/109 (91.7) Resistant to Ampicillin 68/103 (66.0) 55/100 (55.0) Ceftazidime 0 0 Streptomycin 69/103 (67.0) 48/100 (48.0) Kanamycin 29/103 (28.2) 23/100 (23.0) Gentamicin 10/103 (9.7) 3/100 (3.0) Chloramphenicol 30/103 (29.1) 14/100 (14.0) Tetracycline 73/103 (70.9) 43/100 (43.0) Nalidixic acid 22/103 (21.4) 3/100 (3.0) Escherichia coli (f) Any 100/109 (91.7) 98/109 (89.9) Resistant to Ampicillin 36/100 (36.0) 34/98 (34.7) Ceftazidime 0 0 Streptomycin 50/100 (50.0) 35/98 (35.7) Kanamycin 10/100 (10.0) 12/98 (12.2) Gentamicin 2/100 (2.0) 0 Chloramphenicol 11/100 (11.0) 9/98 (9.2) Tetracycline 52/100 (52.0) 23/98 (23.5) Cotrimoxazole 37/100 (37.0) 12/98 (12.2) Nalidixic acid 11/100 (11.0) 0 Staphylococcus aureus 4/109 (3.7) 2/109 (1.8) Yeasts 19 (g)/109 (17.4) 18 (h)/109 (17.4) Microorganisms Prevalence ratio 95 % CI p value Enterococci Any 0.89 0.75 to 1.05 0.21 Resistant to Erythromycin 0.93 0.70 to .24 0.62 Vancomycin 0.68 0.26 to 1.77 0.42 Enterobacteria (d) Any 1.03 0.96 to 1.10 0.58 Resistant to Ampicillin 1.20 0.96 to 1.50 0.11 Ceftazidime NA (e) NA NA Streptomycin 1.40 1.09 to 1.78 <0.01 Kanamycin 1.22 0.76 to 1.96 0.40 Gentamicin 3.24 0.92 to 11.42 0.05 Chloramphenicol 2.08 1.17 to 3.68 <0.01 Tetracycline 1.65 1.27 to 2.13 <0.01 Nalidixic acid 7.12 2.20 to 23.0 <0.01 Escherichia coli (f) Any 1.02 0.94 to 1.10 0.64 Resistant to Ampicillin 1.04 0.71 to 1.51 0.85 Ceftazidime NA NA NA Streptomycin 1.40 1.01 to 1.95 0.04 Kanamycin 0.82 0.37 to 1.80 0.62 Gentamicin NA NA 0.99 Chloramphenicol 1.20 0.52 to 2.76 0.67 Tetracycline 2.22 1.48 to 3.32 <0.01 Cotrimoxazole 3.02 1.68 to 5.44 <0.01 Nalidixic acid NA NA <0.01 Staphylococcus aureus 2.0 0.37 to 10.69 0.68 Yeasts 1.06 0.59 to 1.90 1.00 (a) Matched fecal samples were available for 109 pig farmers and nonfarmer pairs only. (b) Enterococcus faecium: 0, E. gallinarum: 6. (c) E. faecium: 2, E. gallinarum: 5, E. casseliflavus: 3. (d) Using direct plating plating on Drigalski agar without or with antimicrobial agents (first technique, see Methods). (e) NA, not applicable. (f) From the predominant fecal flora (second technique, see Methods). (g) Candida albicans: 1, Geotrichum sp.: 15, C. glabrata: 2, Rhodolulora sp.: 1. (h) C. albicans: 2, Geotrichum sp.: 14, Saccharomyces cerevesia: 2. Table 5. Frequency of use of masks and gloves by 113 pig farmers during selected farming activity No. (%) using (a) No. (%) with Activity that activity Masks Gloves Food preparation, daily or 109 (96) 4 (3.6) 8 (7.3) often Manual food distribution, 78 (69) 4 (5.2) 5 (6.4) handling, or mixing Handling of pig feces, 87 (77) 2 (2.3) 7 (8.0) daily or often Antibiotic administration 112 (99) 4 (3.5) 9 (8.0) to animals (a) During that activity.
We thank J. Bordet, R. Camus, R. Carozzani, M.F. Darchy, N. Fily, P. Gales, J. Gaudon, M. Harrewyn, C. Le Henaff, Y. Koskas, E. Lecocq, A. Lozach, J.L. Mary, P.Morriseau, N. N'Guyen, J.C. Presle, D. Peron, J. Ribbe, M. Roy, J. Roze, G. Savatier, who recruited the study participants, interviewed them, and obtained the primary samples; M. Goldberg, H. de Valk, M. Valenciano, and D. Daube for discussion; V. Jarlier and l'Observatoire de l'Epidemiologie de la Resistance aux Antibiotiques for providing a questionnaire during the investigation of contacts from methicillin-resistant Staphylococcus aureus carriers; and G.B. Pier for critical reading of the manuscript.
This work was supported in part by contract AC003E from the Ministere de l'Amenagement du Territoire et de l'Environnement (Programme de Recherche Environnement et Sante 1999) and by a grant from Mutualite Sociale Agricole, France. This work was presented in part at the 32nd ICAAC September 2002, San Diego, California.
(1.) Levy SB. Ecology of antibiotic resistance determinants. In: Press CSHL, editor. Antibiotic resistance genes: ecology, transfer and expression. New York: Cold Spring Harbor Press; 1986. p. 1730.
(2.) Summers AO. Generally overlooked fundamentals of bacterial genetics and ecology. Clin Infect Dis 2002;34(Suppl 3):S85-92.
(3.) Dowson C, Coffey T, Spratt B. Origin and molecular epidemiology of penicillin-binding-protein-mediated resistance to beta-lactam antibiotics. Trends Microbiol 1994;2:361-6.
(4.) Tauxe RV, Cavanagh TR, Cohen ML. Interspecies gene transfer in viva producing an outbreak of multiply resistant shigellosis. J Infect Dis 1989;160:1067-70.
(5.) Hunter JE, Shelley JC, Walton JR, Hart CA, Bennett M. Apramycin resistance plasmids in Escherichia coli: possible transfer to Salmonella typhimurium in calves. Epidemiol Infect 1992;108:271-8.
(6.) Gast RK, Stephens JF. In vivo transfer of antibiotic resistance to a strain of Salmonella arizonae. Poult Sci 1986;65:270-9.
(7.) Cohen ML. Epidemiology of drug resistance: implications for a post-antimicrobial era. Science 1992;257:1050-5.
(8.) Moulin G. Surveillance of antimicrobial consumption: activities in France (Agence Nationale du Medicament Veterinaire). In: 2nd International Conference of the Office International des Epizoosties, 2001; Paris; 2001.
(9.) Corpet DE. Antibiotic resistance from food. N Engl J Med 1988;318:1206-7.
(10.) Perrier-Gros-Claude J, Courrier P, Breard J, Vignot J, Masseront T, Garin D, et al. Enterocoques resistants aux glycopeptides dans les viandes. Bulletin Epidemiologique Hebdomadaire 1998:50-1.
(11.) Marshall B, Petrowski D, Levy S. Inter- and intraspecies spread of Escherichia coli in a farm environment in the absence of antibiotic usage. Proc Natl Acad Sci U S A 1990;87:660-13.
(12.) Nijsten R, London N, van den Bogaard A, Stobberingh E. Resistance in faecal Escherichia coli isolated from pigfarmers and abattoir workers. Epidemiol Infect 1994; 113:45-52.
(13.) Nijsten R, London N, van den Bogaard A, Stobberingh E. Antibiotic resistance among Escherichia coli isolated from faecal samples of pig farmers and pigs. J Antimicrob Chemother 1996;37:1131-40.
(14.) Stobberingh E, van den Bogaard A, London N, Driessen C, Top J, Willems R. Enterococci with glycopeptide resistance in turkeys, turkey farmers, turkey slaughterers, and (sub)urban residents in the south of The Netherlands: evidence for transmission of vancomycin resistance from animals to humans? Antimicrob Agents Chemother 1999;43:2215-21.
(15.) Chachaty E, Youssef MT, Bourneix C, Andremont A. Shedding of antibiotic-resistant members of the family Enterobacteriaceae in healthy residents of France and Jordan. Res Microbial 1995;146:175-82.
(16.) ATC i. ATC index with DDDs. Oslo: WHO Collaborating Centre for Drug Statistics Methodology; 1999.
(17.) Bellon O, Cavallo JD, Roussel-Delvallez M, Pean Y, Weber P. Antibiotic resistance outside the hospital. La Lettre de l'Infectiologue 2000;25:158-66.
(18.) Communique. Communique du Comite de l'Antibiogramme de la Societe Francaise de Microbiologie. Paris. [accessed April 2002]. Available from: http://www.sfm.asso.fr
(19.) Satake S, Clark N, Rimland D, Nolte FS, Tenover FC. Detection of vancomycin-resistant enterococci in fecal samples by PCR. J Clin Microbial 1997;35:2325-30.
(20.) Roger M, Faucher MC, Forest P, St-Antoine P, Coutlee F. Evaluation of a vanA-specific PCR assay for detection of vancomycin-resistant Enterococcus faecium during a hospital outbreak. J Clin Microbial 1999;37:3348-9.
(21.) Dutka-Malen S, Evers S, Courvalin P. Detection of glycopeptide resistance genotypes and identification to the species level of clinically relevant enterococci by PCR. J Clin Microbial 1995;33:1434.
(22.) Lester S, Del Pilar Pla M, Wang F, Perez Schaeli I, O'Brien T. The carriage of Escherichia coli resistant to antimicrobial agents by healthy children in Boston, Caracas, Venezuela, and in Qin Pu, China. N Engl J Med 1990;323:285-9.
(23.) Hennekens CH, Buring JE. Epidemiology in medicine. In: Cie Ba, editor. Boston: Little, Brown; 1987. p. 77-96.
(24.) Glantz SA. Primer of biostatistics. New York: McGraw Hill; 1981:87-8.
(25.) Rothman KJ. No adjustments are needed for multiple comparisons. Epidemiology 1990;1:43-6.
(26.) Savitz DA, Olshan AF. Multiple comparisons and related issues in the interpretation of epidemiologic data. Am J Epidemiol 1995; 142:904-8.
(27.) Miller RG. Simultaneous statistical inference. Berlin: Springer Verlag; 1981. p. 6-8.
(28.) Kluytmans J, van Belkum A, Verbrugh H. Nasal carriage of Staphylococcus aureus: epidemiology, underlying mechanisms, and associated risks. Clin Microbiol Rev 1997;10:505-20.
(29.) Maiden MC. Horizontal genetic exchange, evolution, and spread of antibiotic resistance in bacteria. Clin Infect Dis 1998;27(Suppl 1):S12-20.
(30.) Levy SB, Marshall B, Schluederberg S, Rowse D, Davis J. High frequency of antimicrobial resistance in human fecal flora. Antimicrob Agents Chemother 1988;32:1801-6.
(31.) Boisivon A, Thibault M, Leclercq R. Colonization by vancomycin-resistant enterococci of the intestinal tract of patients in intensive care units from French general hospitals. Clin Microbial Infect 1997;3:175-9.
(32.) Use of antibiotics in animal feed. Official Journal of the European Communities, editor. Friday 15 May 1998, Council resolution of 8 June 1999 on antibiotic resistance: a strategy against the microbial threat, p. C 195/1-3.
(33.) Bories G, Louisot P. Rapport concernant l'utilisation d'antibiotiques comme facteurs de croissance en alimentation animale: Mission conjoine du Ministere Suedois de l'Agriculture, de la Peche el de l'Alimentation etdu Secretariat a la Sante et a la Securite Sociale du 30 Mai 1997; 1998. Available from: http://www.agruculture.gouv.fr/medi/edut/rapp-Boris.doc
(34.) Cremieux AC, Muller-Serieys C, Panhard X, Delatour F, Tchimichkian M, Mentre F, et al. Emergence of resistance in normal human aerobic commensal flora during telithromycin and amoxicillin-clavulanic acid treatments. Antimicrob Agents Chemother 2003;47:2030-5.
(35.) Sullivan A, Edlund C, Nord CE. Effect of antimicrobial agents on the ecological balance of human microflora. Lancet Infect Dis 2001;1:101-4.
(36.) Fornasini M, Reves RR, Murray BE, Morrow AL, Pickering LK. Trimethoprim-resistant Escherichia coli in households of children attending day care centers. J Infect Dis 1992;166:326-30.
(37.) DANMAP. Use of antimicrobial agents and occurrence of antimicrobial resistance in bacteria from food animals, food and humans in Denmark. 2002. ISNN 1600-2032. Available from: http://www.vetinst.dk
Dr. Aubry-Damon is a specialist in medical microbiology. She works in the Department of Infectious Diseases of the National Institute for Public Health, Saint Maurice, France. Her primary research interest is the surveillance of bacterial resistance to antimicrobial agents.
Address for correspondence: Antoine Andremont, Laboratoire de Bacteriologie, Groupe Hospitalier Bichat-Claude Bernard, 46 rue Huchard--75018 Paris, France; tax: 33 1 40 25 85 81; email: firstname.lastname@example.org
Helene Aubry-Damon, * Karine Grenet, ([dagger]) Penda Sall-Ndiaye, ([double dagger]) Didier Che, * Eugenio Cordeiro, * Marie-Elisabeth Bougnoux, ([paragraph]) Emma Rigaud, ([double dagger]) Yann Le Strat, * Veronique Lemanissier, * Laurence Armand-Lefevre, ([dagger]) Didier Delzescaux, ([section]) Jean-Claude Desenclos, * Michel Lienard, ([double dagger]) and Antoine Andremont ([dagger])
* National Institute for Public Health, Saint-Maurice, France; ([dagger]) Bichat Hospital, Assistance Publique, Paris, France; ([double dagger]) National Mutualite Sociale Agricole, Bagnolet, France; ([section]) National Federation of Cattle and Pig Raisers, Paris, France; and ([paragraph]) Ambroise Hospital, Assistance Publique, Paris, France
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|Publication:||Emerging Infectious Diseases|
|Date:||May 1, 2004|
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