• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of jcmPermissionsJournals.ASM.orgJournalJCM ArticleJournal InfoAuthorsReviewers
J Clin Microbiol. Dec 2004; 42(12): 5578–5581.
PMCID: PMC535250

Detection of Methicillin-Resistant Staphylococcus aureus Directly from Nasal Swab Specimens by a Real-Time PCR Assay


Screening for colonization with methicillin-resistant Staphylococcus aureus (MRSA) is a key aspect of infection control to limit the nosocomial spread of this organism. Current methods for the detection of MRSA in clinical microbiology laboratories, including molecularly based techniques, require a culture step and the isolation of pure colonies that result in a minimum of 20 to 24 h until a result is known. We describe a qualitative in vitro diagnostic test for the rapid detection of MRSA directly from nasal swab specimens (IDI-MRSA; Infectio Diagnostic, Inc., Sainte-Foy, Québec, Canada), based upon a real-time PCR and direct detection of MRSA via amplicon hybridization with a fluorogenic target-specific molecular beacon probe. Samples from 288 patients were analyzed for the presence of MRSA with the IDI-MRSA assay, compared to detection by either direct plating or enrichment broth selective culture methods. The diagnostic values for this MRSA screening method were 91.7% sensitivity, 93.5% specificity, 82.5% positive predictive value, and 97.1% negative predictive value when compared to culture-based methods. The time from the start of processing of specimen to result was approximately 1.5 h. In our hands, the IDI-MRSA assay is a sensitive and specific test for detection of nasal colonization with MRSA and providing for same-day results, allowing more efficient and effective use of infection control resources to control MRSA in health care facilities.

Methicillin-resistant Staphylococcus aureus (MRSA) has been steadily increasing as a cause of infections among hospitalized patients in the United States since it was first reported in the 1960s. According to the National Nosocomial Infection Surveillance System of the Centers for Disease Control and Prevention, in 2002 MRSA accounted for 57.1% of all S. aureus isolates obtained from patients in more than 300 participating intensive care units throughout the United States (20). Large outbreaks of MRSA in other institutions, such as correctional facilities (4, 22), and among otherwise healthy individuals in the community (15) raise the concern that this organism is spreading outside of its traditional role as a health care-related pathogen. Infections caused by MRSA result in increased lengths of hospital stay, health care costs, morbidity, and mortality (10, 21, 24) compared to those caused by methicillin-sensitive strains.

Infection control measures, such as placing hospitalized patients colonized or infected with MRSA in contact precautions (i.e., the use of gowns and gloves), have been demonstrated to limit the spread of this pathogen (5, 13). The use of surveillance cultures (e.g., anterior nares, axillae, and perineum) greatly improves the detection of MRSA colonization compared to clinical cultures alone (7). The anterior nares is the most frequent site of MRSA colonization, with a single culture from this site having a sensitivity of approximately 85% (7, 26).

Methicillin resistance in Staphylococcus spp. is primarily mediated by the mecA gene, encoding penicillin-binding protein 2a (PBP2a). This protein has reduced affinity for β-lactam antibiotics. Because the mecA gene is heterogeneously expressed in vitro (6), selective media are necessary to facilitate recovery of MRSA in culture. The time from culture inoculation to identification of MRSA is typically 48 h, with some methods taking as long as 96 h (25). Furthermore, the sensitivity of any single selective medium method ranges between 65 and 100% (25). Several techniques to shorten the time to identification of MRSA in the laboratory have been developed in the last decade, including slide latex agglutination assays to detect PBP2a (2, 17, 19, 30, 32), a colorimetric cycling probe assay to directly detect the mecA gene (1, 16, 31), and real-time PCR methods to detect the mecA gene (3, 8, 9, 14, 16, 23, 27) in conjunction with S. aureus-specific genome fragments, such as nuc (8, 9, 16) and sa442 (23, 27). While these assays are sensitive in detecting MRSA, they are unable to distinguish MRSA from mecA-positive strains of coagulase-negative Staphylococcus spp. in mixed specimens, such as those obtained from the anterior nares, and therefore still require initial culture and identification steps.

IDI-MRSA (Infectio Diagnostic, Inc., Sainte-Foy, Québec, Canada) is a qualitative in vitro diagnostic test for the rapid detection of MRSA directly from nasal swabs. The test utilizes the real-time PCR method for the amplification of an MRSA-specific DNA sequence recovered from clinical samples and fluorogenic target-specific hybridization with a molecular beacon probe (29) for the detection of the amplified MRSA DNA. The sequences targeted in this assay are within SCCmec, the mobile genetic element which harbors the mecA gene (12), and orfX, a highly conserved open reading frame in S. aureus which is the site of SCCmec integration into the genome; the exact target sequences have been described previously (11). In the presence of these sequences, target-specific primers within the assay will bind and generate an MRSA-specific amplicon during the PCR, which is then detected by a complementary molecular beacon probe. We describe the validation of this assay for the detection of MRSA from swabs obtained from the anterior nares of hospitalized patients, compared to detection of MRSA by either of two culture-based methods.


Study enrollment and collection of clinical specimens.

Study subjects were selected from inpatients at Barnes-Jewish Hospital, a 1,442-bed academic, tertiary care hospital in St. Louis, Mo. Subjects were selected from both new and currently admitted patients. Patients were considered for inclusion in the study if they met any of the following criteria: (i) prior MRSA infection or colonization, (ii) current hospital stay exceeding 3 days, or (iii) known colonization or infection with a hospital-acquired pathogen (e.g., vancomycin-resistant Enterococcus spp.). These criteria were chosen to select a patient population at high risk for MRSA nasal colonization. Patients were excluded from the study if they had received treatment with intranasal mupirocin or polysporin in the previous 14 days, treatment with oral antimicrobials for the purpose of eradicating MRSA colonization within the past 14 days (including oral rifampin therapy for any reason), or had contraindications to nasal sampling. After written informed consent was obtained, each patient had a specimen collected from the nares with a dry, unmoistened swab (Venturi Transystem; Copan Diagnostics, Corona, Calif.). The tip of the collection swab was inserted approximately 1 in. (2.56 cm) into the nares and rolled five times in each nostril. Collected specimens were transported and stored at room temperature. Cultures were inoculated and specimens were processed for PCR analysis within 24 h of being collected (time to culture inoculation: median, 1.7 h; range, 0.3 to 17.9 h; time to processing for PCR, median, 14.4 h; range, 2.7 to 19.0 h). Each collection swab was initially inoculated into S. aureus selective agar and then into a buffer solution for the IDI-MRSA assay and finally into S. aureus selective broth medium (see below). This study was approved by the Washington University Human Studies Committee.

Selective media and culture conditions.

Mannitol salt agar plates (Becton Dickinson, Cockeysville, Md.) were inoculated directly with specimen swabs prior to testing of the same swab with the IDI-MRSA assay. The mannitol salt agar plates were incubated for 24 to 48 h at 35°C and examined for growth. Strains that produced yellow colonies on mannitol salt agar screen were confirmed as S. aureus with Gram stain, 3% catalase testing, and coagulase testing with the Staph Latex agglutination assay (LifeSign, Somerset, N.J.). After the specimen swabs were processed for testing with the IDI-MRSA assay, the swabs were used to inoculate an enrichment broth medium containing tryptic soy broth and 6.5% sodium chloride (Remel, Lenexa, Kans.). The enrichment broth was incubated overnight at 35°C and then subcultured to 5% sheep blood agar (Becton Dickinson) for 18 to 24 h at 35°C. Colonies on the 5% sheep blood agar plates consistent with those for S. aureus were confirmed as previously described.

Detection of MRSA by culture methods.

Confirmed S. aureus isolates were subcultured from the 5% sheep's blood agar plates onto oxacillin screen agar containing 6.0 μg of oxacillin per ml (Becton Dickinson). Plates were incubated at 35°C for 18 to 24 h and examined for evidence of growth. Strains showing distinct growth were considered to be methicillin resistant.

Processing specimen swabs with the IDI-MRSA assay.

Specimens were processed for PCR analysis per the manufacturer's instructions. Cell lysis and DNA preparation were achieved with a set of two tubes per patient sample provided with the IDI-MRSA kit. Nasal swabs were initially vortexed in a tube containing 1 ml of sample buffer, and 850 μl of this was transferred to a lysis tube. Following centrifugation at 21,000 × g for 5 min and removal of the supernatant, 50 μl of sample preparation buffer was then added to each lysis tube and bacterial cell lysis was achieved by vortexing for 5 min. Lysis tubes were then centrifuged, heated for 2 min at 95°C, and stored at 4°C prior to analysis by real-time PCR.

Real-time PCR using the IDI-MRSA assay.

PCR tubes containing the lyophilized master mix were reconstituted with diluent, and specimen DNA was added. The PCR was performed with a Smart Cycler II device (Cepheid, Sunnyvale, Calif.). The run time for the PCR component of the assay was 45 min. To ensure that the PCR takes place, the IDI-MRSA assay includes an internal control DNA sequence with complementary primers that is incorporated into each sample. The internal control used is based upon a previously described linearized plasmid (11) and consists of a 335-bp DNA fragment composed of a 277-bp non-MRSA sequence flanked by the sequences of the meciv511 and mecv492 primers. This fragment was cloned into the pCR2.1 vector (Invitrogen, Burlington, Ontario, Canada) and linearized for use in the assay. External positive and negative controls were included with each PCR run. PCRs of individual specimens were repeated if the internal control was invalid due to the presence of inhibitors or if the positive or negative controls were invalid.

Data analysis.

Statistical analysis was performed with SPSS for Windows, version 11.0 (SPSS, Inc., Chicago, Ill.). Ninety-five percent confidence intervals (CI) for sensitivity and specificity were calculated by standard methods (28). In the case of discordant results between culture methods and the IDI-MRSA assay, the assay was repeated and the results were noted; however, for purposes of calculating sensitivity and specificity, only the initial result was considered.


Nasal swab specimens were obtained from 290 patients between June and September 2003. Two patients were subsequently found to be ineligible for the study due to concurrent rifampin-containing therapy for mycobacterial infections. Of the samples from the remaining 288 patients, 2 (0.7%) with negative internal controls due to the presence of PCR inhibitors were examined again. Both samples were resolved upon repeat testing. Thus, 288 specimens were valid for determining sensitivity and specificity. Sixty-four (22.2%) of the source patients had a past history of MRSA infection of colonization, and 203 (70.5%) had received oral or intravenous antimicrobial therapy within the 2 weeks prior to testing.

Of the 288 specimens tested, 72 (25%) were positive for MRSA by direct plating or broth enrichment methods. Fifty-nine (20.5%) specimens were positive for MRSA by both culture methods, while 7 (2.4%) specimens were MRSA positive only by broth enrichment, and 6 (2.1%) were positive by the direct plating method alone.

A comparison of the IDI-MRSA assay to culture methods for the detection of methicillin-resistant S. aureus is shown in Table Table1.1. Compared to the direct plating method alone, the assay had a sensitivity of 98.5% (95% CI, 95.5 to 100%) and a specificity of 92.8% (95% CI, 89.4 to 96.2%). However, the direct plating method alone detected only 65 of 72 (90.3%) patients with nasal colonization with MRSA. Likewise, the enrichment broth method detected 66 (91.7%) of MRSA nasal carriers. When compared to either culture method, the IDI-MRSA assay had a sensitivity of 91.7% (95% CI, 85.3 to 98.1%) and a specificity of 93.5% (95% CI, 90.2 to 96.8%), with a positive predictive value of 82.5% and negative predictive value of 97.1%. To examine the effects of delayed processing on assay sensitivity, when specimens that were processed for PCR analysis at greater than the median time after collection (14.4 h; n = 145) were considered, the sensitivity and specificity of the assay were 90.0 and 96.5%, respectively. Typically, 8 to 10 specimens were batched for processing and analyzed with external positive and negative control samples per each run. The time from specimen centrifugation to generation of results for this number of specimens was approximately 1.5 h.

Sensitivity and specificity of the IDI-MRSA real-time PCR assay compared to culture methods for detection of MRSA from nasal swabs


Rapid identification of MRSA colonization is critical to the effectiveness of infection control, with delays in detection resulting in either late institution of infection control measures and resultant occult transmission of MRSA between patients or unnecessary contact precautions being applied to high-risk patients, resulting in increased hospital cost. In our hands, the IDI-MRSA assay demonstrated a sensitivity and specificity above 90% for the detection of MRSA nasal colonization compared to two selective culturing methods. The assay can be performed by a single technologist, after receiving appropriate training, and allows same-day results with batching of specimens. The Smart Cycler system used in this study consisted of a single unit that can run 16 samples at once; however, up to six units per controller can be used, allowing 96 samples to be tested simultaneously.

Previous real-time PCR assays (8, 14, 16, 23, 27) have demonstrated the capability of rapidly detecting MRSA from culture. Reischl et al. (23) reported a duplex assay for mecA and the S. aureus-specific sa442 genome fragments using paired FRET probes with a Light Cycler (Roche Diagnostics Corp., Indianapolis, Ind.) real-time PCR instrument. They reported 100% sensitivity and specificity for detecting MRSA from pure colonies. Elsayed et al. (8) used a duplex molecular beacon-based real-time PCR assay containing primers and molecular beacon probes to sequences within the mecA gene and an S. aureus-specific nuc gene. The authors tested 181 strains, including methicillin-sensitive and -resistant S. aureus, methicillin-sensitive and resistant coagulase-negative Staphylococcus spp., and nonstaphylococcus bacteria, and reported 100% sensitivity and specificity for this assay in detecting and differentiating Staphylococcus spp. from pure strain isolates. However, neither of the described assays was able to differentiate methicillin-sensitive S. aureus from methicillin-resistant coagulase-negative Staphylococcus spp. in primary specimens where both of these organisms could coexist, such as the anterior nares. By utilizing primer sequences for SCCmec and orfX regions, an MRSA-specific amplicon is generated, which is then detected by a complementary molecular beacon probe. Theoretically, other specimens (i.e., wound, blood, and perineum) could be directly tested for the presence of MRSA using this assay, but this would require further validation.

The assay in our hands was not 100% sensitive or specific, compared to prior real-time PCR assays performed on pure culture isolates (8, 23). Six of the samples that were positive by at least one of the culture methods were negative by the IDI-MRSA assay. This was not due to the presence of inhibitors to the PCR, as the internal control in each of these tubes was positive. Four of these culture-positive, PCR assay-negative specimens were available for additional testing from saved broth cultures. S. aureus was isolated from all four specimens by inoculation of 5% sheep blood agar plates and identification methods described above. Three of these specimens were found to grow on subculture to oxacillin screen agar and therefore were felt to represent phenotypic MRSA. The presence of the mecA gene in these three isolates was examined with a mecA gene-specific PCR assay described by Martineau et al. (18); all three isolates were negative for the mecA gene, suggesting that methicillin resistance in these isolates was mediated by methods other than PBP2a, such as hyperproduction of β-lactamase or modified PBP genes (6). Other potential explanations for why the assay failed to detect MRSA in false-negative PCR assay samples include possible variability in either the SCCmec or orfX sequences that did not allow amplification with the panel of primers in the assay or the possibility that the number of MRSA organisms present in the specimens was below the limit of detection for the assay. Conversely, 14 specimens were positive for MRSA by PCR assay and negative by either culture method. This may be due to the known limitations in sensitivity of selective culture methods in detecting MRSA from nasal swabs (25). Cross-contamination of specimens during preparation is also a possibility—3 of the 14 samples were PCR negative upon repeated testing with saved lysate solution. We also noted that the broth enrichment culture method in this study was as sensitive as the direct plating method used to detect MRSA, in contrast to previous studies (25). This might have been due to the order of inoculation in our study (i.e., the broth was inoculated after the direct plating and processing for the PCR assay).

In summary, the IDI-MRSA assay is a sensitive and specific test for the detection of MRSA nasal colonization directly from a swab specimen, without the need for an initial culture. This assay can be performed by a microbiologist technician with minimal additional training and allows same-day results, even with batching of specimens. This promises to improve the efficiency and effectiveness of measures to control the spread of this resistant organism throughout health care facilities.


This project was funded in part by a research grant from Infectio Diagnostic, Inc., who had no part in the recruitment of patients or analysis of data for this study.

We thank Godson Onwubiko for enrolling patients and obtaining specimens. We also acknowledge Cherie Hill and Stacy Leimbach for the management of research data for this study.


1. Bekkaoui, F., J. P. McNevin, C. H. Leung, G. J. Peterson, A. Patel, R. S. Bhatt, and R. N. Bryan. 1999. Rapid detection of the mecA gene in methicillin resistant staphylococci using a colorimetric cycling probe technology. Diagn. Microbiol. Infect. Dis. 34:83-90. [PubMed]
2. Brown, D. F., and E. Walpole. 2001. Evaluation of the Mastalex latex agglutination test for methicillin resistance in Staphylococcus aureus grown on different screening media. J. Antimicrob. Chemother. 47:187-189. [PubMed]
3. Carroll, K. C., R. B. Leonard, P. L. Newcomb-Gayman, and D. R. Hillyard. 1996. Rapid detection of the staphylococcal mecA gene from BACTEC blood culture bottles by the polymerase chain reaction. Am. J. Clin. Pathol. 106:600-605. [PubMed]
4. Centers for Disease Control and Prevention. 2003. Outbreaks of community-associated methicillin-resistant Staphylococcus aureus skin infections—Los Angeles County, California, 2002-2003. Morb. Mortal. Wkly. Rep. 52:88. [PubMed]
5. Chaix, C., I. Durand-Zaleski, C. Alberti, and C. Brun-Buisson. 1999. Control of endemic methicillin-resistant Staphylococcus aureus: a cost-benefit analysis in an intensive care unit. JAMA 282:1745-1751. [PubMed]
6. Chambers, H. F. 1997. Methicillin resistance in staphylococci: molecular and biochemical basis and clinical implications. Clin. Microbiol. Rev. 10:781-791. [PMC free article] [PubMed]
7. Coello, R., J. Jimenez, M. Garcia, P. Arroyo, D. Minguez, C. Fernandez, F. Cruzet, and C. Gaspar. 1994. Prospective study of infection, colonization and carriage of methicillin-resistant Staphylococcus aureus in an outbreak affecting 990 patients. Eur. J. Clin. Microbiol. Infect. Dis. 13:74-81. [PubMed]
8. Elsayed, S., B. L. Chow, N. L. Hamilton, D. B. Gregson, J. D. Pitout, and D. L. Church. 2003. Development and validation of a molecular beacon probe-based real-time polymerase chain reaction assay for rapid detection of methicillin resistance in Staphylococcus aureus. Arch. Pathol. Lab. Med. 127:845-849. [PubMed]
9. Fang, H., and G. Hedin. 2003. Rapid screening and identification of methicillin-resistant Staphylococcus aureus from clinical samples by selective-broth and real-time PCR assay. J. Clin. Microbiol. 41:2894-2899. [PMC free article] [PubMed]
10. Harbarth, S., O. Rutschmann, P. Sudre, and D. Pittet. 1998. Impact of methicillin resistance on the outcome of patients with bacteremia caused by Staphylococcus aureus. Arch. Intern. Med. 158:182-189. [PubMed]
11. Huletsky, A., R. Giroux, V. Rossbach, M. Gagnon, M. Vaillancourt, M. Bernier, F. Gagnon, K. Truchon, M. Bastien, F. J. Picard, A. van Belkum, M. Ouellette, P. H. Roy, and M. G. Bergeron. 2004. New real-time PCR assay for rapid detection of methicillin-resistant Staphylococcus aureus directly from specimens containing a mixture of staphylococci. J. Clin. Microbiol. 42:1875-1884. [PMC free article] [PubMed]
12. Ito, T., Y. Katayama, and K. Hiramatsu. 1999. Cloning and nucleotide sequence determination of the entire mec DNA of pre-methicillin-resistant Staphylococcus aureus N315. Antimicrob. Agents Chemother. 43:1449-1458. [PMC free article] [PubMed]
13. Jernigan, J. A., M. G. Titus, D. H. Groschel, S. Getchell-White, and B. M. Farr. 1996. Effectiveness of contact isolation during a hospital outbreak of methicillin-resistant Staphylococcus aureus. Am. J. Epidemiol. 143:496-504. (Erratum, 143:1079). [PubMed]
14. Killgore, G. E., B. Holloway, and F. C. Tenover. 2000. A 5′ nuclease PCR (TaqMan) high-throughput assay for detection of the mecA gene in staphylococci. J. Clin. Microbiol. 38:2516-2519. [PMC free article] [PubMed]
15. Lindenmayer, J. M., S. Schoenfeld, R. O'Grady, and J. K. Carney. 1998. Methicillin-resistant Staphylococcus aureus in a high school wrestling team and the surrounding community. Arch. Intern. Med. 158:895-899. [PubMed]
16. Louie, L., J. Goodfellow, P. Mathieu, A. Glatt, M. Louie, and A. E. Simor. 2002. Rapid detection of methicillin-resistant staphylococci from blood culture bottles by using a multiplex PCR assay. J. Clin. Microbiol. 40:2786-2790. [PMC free article] [PubMed]
17. Love, J. B., C. A. Wright, D. H. Hooke, W. G. Parkin, P. Bills, and R. Baird. 1992. Exfoliative dermatitis as a risk factor for epidemic spread of methicillin resistant Staphylococcus aureus. Intensive Care Med. 18:189. [PubMed]
18. Martineau, F., F. J. Picard, N. Lansac, C. Ménard, P. H. Roy, M. Ouellette, and M. G. Bergeron. 2000. Correlation between the resistance genotype determined by multiplex PCR assays and the antibiotic susceptibility patterns of Staphylococcus aureus and Staphylococcus epidermidis. Antimicrob. Agents Chemother. 44:231-238. [PMC free article] [PubMed]
19. Nakatomi, Y., and J. Sugiyama. 1998. A rapid latex agglutination assay for the detection of penicillin-binding protein 2′. Microbiol. Immunol. 42:739-743. [PubMed]
20. National Nosocomial Infections Surveillance System. 2003. National Nosocomial Infections Surveillance (NNIS) System report, data summary from January 1992 through June 2003, issued August 2003. Am. J. Infect. Control 31:481-498. [PubMed]
21. Niclaes, L., F. Buntinx, F. Banuro, E. Lesaffre, and J. Heyrman. 1999. Consequences of MRSA carriage in nursing home residents. Epidemiol. Infect. 122:235-239. [PMC free article] [PubMed]
22. Pan, E. S., B. A. Diep, H. A. Carleton, E. D. Charlebois, G. F. Sensabaugh, B. L. Haller, and F. Perdreau-Remington. 2003. Increasing prevalence of methicillin-resistant Staphylococcus aureus infection in California jails. Clin. Infect. Dis. 37:1384-1388. [PubMed]
23. Reischl, U., H.-J. Linde, M. Metz, B. Leppmeier, and N. Lehn. 2000. Rapid identification of methicillin-resistant Staphylococcus aureus and simultaneous species confirmation using real-time fluorescence PCR. J. Clin. Microbiol. 38:2429-2433. [PMC free article] [PubMed]
24. Rubin, R. J., C. A. Harrington, A. Poon, K. Dietrich, J. A. Greene, and A. Moiduddin. 1999. The economic impact of Staphylococcus aureus infection in New York City hospitals. Emerg. Infect. Dis. 5:9-17. [PMC free article] [PubMed]
25. Safdar, N., L. Narans, B. Gordon, and D. G. Maki. 2003. Comparison of culture screening methods for detection of nasal carriage of methicillin-resistant Staphylococcus aureus: a prospective study comparing 32 methods. J. Clin. Microbiol. 41:3163-3166. [PMC free article] [PubMed]
26. Sewell, D. L., S. A. Potter, C. M. Jacobson, L. J. Strausbaugh, and T. T. Ward. 1993. Sensitivity of surveillance cultures for the detection of methicillin-resistant Staphylococcus aureus in a nursing-home-care unit. Diagn. Microbiol. Infect. Dis. 17:53-56. [PubMed]
27. Shrestha, N. K., M. J. Tuohy, G. S. Hall, C. M. Isada, and G. W. Procop. 2002. Rapid identification of Staphylococcus aureus and the mecA gene from BacT/ALERT blood culture bottles by using the LightCycler system. J. Clin. Microbiol. 40:2659-2661. [PMC free article] [PubMed]
28. Szklo, M., and F. J. Nieto. 2003. Epidemiology: beyond the basics. Aspen Publishers, Inc., Gaithersburg, Md.
29. Tyagi, S., D. P. Bratu, and F. R. Kramer. 1998. Multicolor molecular beacons for allele discrimination. Nat. Biotechnol. 16:49-53. [PubMed]
30. van Griethuysen, A., M. Pouw, N. van Leeuwen, M. Heck, P. Willemse, A. Buiting, and J. Kluytmans. 1999. Rapid slide latex agglutination test for detection of methicillin resistance in Staphylococcus aureus. J. Clin. Microbiol. 37:2789-2792. [PMC free article] [PubMed]
31. van Leeuwen, W. B., D. E. Kreft, and H. Verbrugh. 2002. Validation of rapid screening tests for the identification of methicillin resistance in staphylococci. Microb. Drug Resist. 8:55-59. [PubMed]
32. van Leeuwen, W. B., C. van Pelt, A. Luijendijk, H. A. Verbrugh, and W. H. F. Goessens. 1999. Rapid detection of methicillin resistance in Staphylococcus aureus isolates by the MRSA-Screen latex agglutination test. J. Clin. Microbiol. 37:3029-3030. [PMC free article] [PubMed]

Articles from Journal of Clinical Microbiology are provided here courtesy of American Society for Microbiology (ASM)
PubReader format: click here to try


Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...