Skip directly to search Skip directly to A to Z list Skip directly to page options Skip directly to site content

Volume 8, Number 7—July 2002


Antibiotic Resistance of Gram-Negative Bacteria in Rivers, United States

Ronald J. Ash*Comments to Author , Brena Mauck*, and Melissa Morgan*
Author affiliations: *Washburn University, Topeka, Kansas, USA;

Suggested citation for this article


Bacteria with intrinsic resistance to antibiotics are found in nature. Such organisms may acquire additional resistance genes from bacteria introduced into soil or water, and the resident bacteria may be the reservoir or source of widespread resistant organisms found in many environments. We isolated antibiotic-resistant bacteria in freshwater samples from 16 U.S. rivers at 22 sites and measured the prevalence of organisms resistant to β-lactam and non β-lactam antibiotics. Over 40% of the bacteria resistant to more than one antibiotic had at least one plasmid. Ampicillin resistance genes, as well as other resistance traits, were identified in 70% of the plasmids. The most common resistant organisms belonged to the following genera: Acinetobacter, Alcaligenes, Citrobacter, Enterobacter, Pseudomonas, and Serratia.

The presence of antibiotic-resistant bacteria in freshwater sources throughout the world has been documented (15). Selection of resistant organisms in nature may result from natural production of antibiotics by soil organisms, runoff from animal feed or crops, or waste products from treated animals or humans (610). Natural reservoirs of resistance genes may provide a source of transferable traits for emerging pathogens (6,11). The prevalence, nature, properties, and origin of such reservoirs in U.S. rivers have not been studied on a national scale. We frequently found organisms resistant to naturally occurring and human-modified antibiotics in U.S. rivers. A large proportion of the resistant organisms were found to contain plasmids with resistance traits.


Sterile pipettes were used to collect triplicate 10-mL water samples at each site. Samples were collected in city limits at all locations; sites were usually 1 mile downstream of the downtown area. Each sample was collected at a depth of approximately 15 cm. Temperature and pH measurements were also made at the time of sampling. All samples, either undiluted or diluted in Luria-Bertani (LB) broth (12), were plated (0.1 mL, spread plate) on LB agar some with and some without ampicillin (150 µg/mL) at the collection site. Ampicillin was used to select for potential β-lactamase producers. Water samples were not stored or concentrated before plating. Plates were incubated at 30°C–32°C for 24 hours before the total number of bacteria and ampicillin-resistant bacteria were estimated. Variations in the number of CFU and ampicillin-resistant CFU did not differ (p=0.01) in a group of the triplicate samples plated at a particular time. Ampicillin-resistant isolates were picked to master LB plus ampicillin plates until further tested against additional antibiotics.

National Committee for Clinical Laboratory Standards (NCCLS) procedures and evaluation methods were used (13). Briefly, isolates were grown in LB plus ampicillin broth until the turbidity of a 0.5 MacFarland standard was reached. Cultures were swabbed on Mueller-Hinton agar, and antibiotic discs (Becton Dickinson and Co., Cockeysville, MD) were added. The antibiotics used were cefotaxime, ceftazidime, amoxicillin plus clavulanic acid, cephalothin, imipenem, kanamycin, streptomycin, chloramphenicol, tetracycline, and ciprofloxacin. MIC were determined with E test strips (AB Biodisk North America, Piscataway, NJ) under NCCLS conditions as described by the manufacturer. Isolates showing complete resistance to at least one antibiotic other than ampicillin were frozen in LB plus 10% dimethyl sulfoxide at -78°C and used as stocks for further testing. Freezing was preferred since isolate storage in the refrigerator for >2 weeks frequently resulted in loss of cultures. Nitrocefin discs (Cefinase, BD Microbiology Systems, Sparks, MD) were placed on bacterial cultures growing on Mueller Hinton agar and observed for the color change indicative of hydrolysis.

Organisms were grown overnight in LB with ampicillin broth with shaking. Two methods were used for every isolate examined: the boiling method (14) and alkaline lysis (15). Agarose gel electrophoresis in 0.7% agarose (GTG, FMC Corp., Rockland, ME) with 1X Tris/acetate/EDTA buffer (12) was used to determine the presence and size of plasmids. Plasmids were purified by removal of unstained gel slices and centrifugal elution through polyester fiberfill plugs (16).

The presence of resistance markers on purified plasmids was determined as follows: electrocompetent Escherichia coli (TOP 10 cells, Invitrogen, Inc., Carlsbad, CA) was mixed with 5 µL of pure plasmid DNA and subjected to 1.8 kV in a Bio-Rad Pulser (Bio-Rad Laboratories, Hercules, CA). Electroporated cells (cells with DNA physically introduced) were mixed with SOC medium (12) and incubated for 60 minutes at 37°C before plating on LB with ampicillin plates. Transformants were picked and checked for additional resistance traits as described above.


The number and range of ampicillin-resistant bacteria recovered at the 22 sites sampled in the past 3 years are shown in Table 1. Fourteen of the rivers were sampled more than once. Considerable variations in the total number of CFU and ampicillin-resistant organisms were encountered. The MIC for ampicillin was >256 for 98% of the ampicillin-resistant organisms tested. This high level of resistance, found in all rivers tested, was not unexpected since initial plating was on LB plates containing 150 µg/mL of the antibiotic. No apparent correlation existed between numbers of culturable or ampicillin-resistant organisms and temperature (range 0°C–28°C) or pH (range 7.2–8.7) in any of the rivers tested (data not shown). The number of resistant isolates growing on MacConkey agar was >90% for most samples. The ampicillin-resistant isolates were predominantly gram-negative nonlactose-fermenters (data not shown). Oxidase testing and biochemical characterization indicated that the major genera of these bacteria were Acinetobacter, Alcaligenes, Citrobacter, Enterobacter, Pseudomonas, and Serratia. Klebsiella and Proteus were also isolated but less frequently than the other organisms.

The resistance of ampicillin-resistant isolates to other β-lactam antibiotics is presented in Table 2. Organisms resistant to cefotaxime, ceftazidime, and imipenem were detected at a number of sites. This finding prompted us to plate water samples on LB medium with cefotaxime (60 µg/mL). Cefotaxime -resistant bacteria were readily isolated from all rivers tested on this selective medium (Table 3). Of these cefotaxime-resistant organisms, 20% to 30% were gram-positive, spore-forming rods, which appeared to belong to the genus Bacillus. Although these gram-positive organisms may be important as reservoirs of resistance genes, only those cefotaxime-resistant isolates growing on MacConkey agar and shown to be gram negative were used for further analysis. Of the gram-negative cefotaxime-resistant organisms, 87% had a cefotaxime MIC >256. The remaining 13% had an MIC >48. Every cefotaxime-resistant isolate was capable of hydrolyzing nitrocefin, indicating the presence of β-lactamase. Many of the cefotaxime-resistant isolates were also resistant to ceftazidime (Table 4). Sixty-one per cent of the ceftazidime-resistant organisms (71 isolates tested) had a ceftazidime MIC >256, while 17% had an MIC of 12 to 192. Most (>80%) of the cefotaxime-resistant and ceftazidime-resistant organisms were identified as Pseudomonas.

The resistance of ampicillin-resistant isolates to non-β–lactam antibiotics is shown in Table 5. Many organisms in the rivers had resistance to at least one antibiotic other than ampicillin, and a substantial fraction were able to survive a number of antibiotics. One gram-negative organism resistant to ciprofloxacin was found in the 3,011 ampicillin-resistant isolates tested. Gram-positive ciprofloxacin-resistant bacteria were more numerous and were readily isolated.

Two different plasmid isolation procedures were used to analyze the isolates resistant to ampicillin and one other antibiotic. Of the 374 isolates, 167 (44%) contained at least one plasmid. This number probably represents a minimal estimate since the methods used may not be optimal for all species encountered. Plasmids ranged in size from 2 kb to >23 kb. Purified plasmids were checked for their ability to transform E. coli. Of the 54 plasmids tested, 38 (70%) contained the gene for ampicillin resistance. Further, 97% of the plasmids with the ampicillin-resistant gene also carried at least one other resistance trait.


We found that culturable antibiotic-resistant bacteria were widespread in nonconcentrated water samples from many U.S. rivers. This finding, in and of itself, is not surprising since the intrinsic resistance of many organisms to antibiotics is well documented (17). Bacteria that are resistant to chemically modified and synthesized antibiotics are also widespread in the environment. The use of selective media resulted in the isolation of gram-negative organisms with high levels of resistance (MIC >256 µg) to the clinically useful β-lactams ampicillin, cefotaxime, and ceftazidime. Organisms resistant to imipenem were also frequently isolated. Nitrocefin hydrolysis data suggest that β-lactamase production is a major mechanism of resistance to ampicillin in river isolates. The resistance of natural isolates to ceftazidime and cefotaxime strongly suggests that these organisms may produce extended-spectrum β-lactamases (ESBL), since resistance to these third-generation cephalosporins is considered the single most important indicator of ESBL (18,19). Alternatively, chromosomal AmpC β-lactamases may be responsible for the resistance of Pseudomonas to cefotaxine and ceftazidime (19). Distinguishing between these possibilities will be important in determining transmissibility of β-lactamase resistance.

Many of the organisms resistant to ampicillin and at least one other antibiotic (40%) harbored plasmids. Although two methods were used to isolate plasmids, some bacteria may have been refractory to these procedures or a large or low copy number plasmids were not observed. Resistance to ampicillin and other antibiotics was plasmid-borne, as indicated by electroporation of cells with purified plasmids.

The results presented here have limitations and must be considered in light of the fact that many aquatic organisms are probably nonculturable (20). The bacteria that cannot be cultivated may be part of the reservoir of resistance genes as well. PCR has been used to identify nonculturable bacteria in stream sediments (21). This technique may be used to identify antibiotic resistance genes in nonculturable organisms as well.

Many of the ampicillin-resistant isolates were also resistant to non-β–lactam antibiotics (Table 5). The frequency with which these organisms were found suggests that characterization of resistance genes and the plasmids on which they reside should provide information about reservoirs for antibiotic resistance in the environment.

Dr. Ash is professor of biology at Washburn University. His research interests include mechanisms of antibiotic resistance.


  1. French GL, Ling J, Chow KL, Mark KK. Occurrence of multiple antibiotic resistance and R-plasmid in gram-negative bacteria isolated from fecally contaminated freshwater streams. Epidemiol Infect. 1987;98:28599.PubMed
  2. Kelch WJ, Lee JS. Antibiotic resistance patterns of gram negative bacteria isolated from environmental sources. Appl Environ Microbiol. 1978;36:4506.PubMed
  3. Niemi M, Sibakov M, Niemala S. Antibiotic resistance among different species of fecal coliforms isolated from water samples. Appl Environ Microbiol. 1983;45:7983.PubMed
  4. Ogan MT, Nwiika DE. Studies on the ecology of aquatic bacteria on the Lower Niger delta: multiple antibiotic resistance among the standard plate count organisms. J Appl Bacteriol. 1993;74:595602.PubMed
  5. Young H-K. Antimicrobial resistance spread in aquatic environments. J Antimicrob Chemother. 1993;31:62735. DOIPubMed
  6. Davies J. Inactivation of antibiotics and the dissemination of resistance genes. Science. 1994;264:37582. DOIPubMed
  7. Levy SB. Antibiotic resistance: an ecological imbalance. In: Chadwick DJ, Goode J, editors. Antibiotic resistance: origins, evolution, selection and spread. Chichester, Great Britian: Wiley and Sons; 1997. p. 1–9.
  8. Witte W. Impact of antibiotic use in animal feeding on resistance of bacterial pathogens in humans. In Chadwick DJ, Goode J, editors. Antibiotic resistance: origins, evolution, selection and spread. Chichester, Great Britian: Wiley and Sons; 1997. p.61–75.
  9. Tenover FC, McGowan JE. Reasons for the emergence of antibiotic resistance. Am J Med Sci. 1996;311:916. DOIPubMed
  10. Witte W. Medical consequences of antibiotic use in agriculture. Science. 1998;279:9967. DOIPubMed
  11. van Elsas JD, Fry J, Hirsch P, Molin S. Ecology of plasmid transfer and spread. In: Thomas CM, editor. The horizontal gene pool. Amsterdam, the Netherlands: Harwood; 2000. p. 175–206.
  12. Sambrook J, Fritsch EF, Maniatis T. Molecular cloning 3. New York: Cold Spring Harbor Press; 1989. p. A1–A2.
  13. National Committee for Clinical Laboratory Standards. Performance standards for antimicrobial disk susceptibility tests M2-A6. Wayne (PA): The Committee; 1997.
  14. Holmes DS, Quigley M. A rapid boiling method for the preparation of bacterial plasmids. Anal Biochem. 1981;114:1937. DOIPubMed
  15. Birnboim HC, Doly J. A rapid alkaline extraction procedure for screening recombinant plasmid DNA. Anal Biochem. 1979;114:1937.
  16. Glenn TC, Glenn SJ. Rapid elution of DNA from agarose gels using polyester plug spin inserts (PEPSIs). Trends Genet. 1994;10:344. DOIPubMed
  17. Quintiliani R Jr, Sahm DF, Courvalin P. Mechanism of resistance to antimicrobial agents. In: Murray PR, Baron EJ, Pfaller MA, Tenover FC, Yolken RH, editors. Manual of clinical microbiology. 7th ed. Washington: ASM Press; 1999. p. 1505–25.
  18. Katsanis GP, Spargo J, Ferraro MJ, Sutton L, Jacoby GA. Detection of Klebsiella pneumoniae and E. coli strains producing extended spectrum beta-lactamases. J Clin Microbiol. 1994;32:6916.PubMed
  19. Livermore DM. Beta-lactamases in laboratory and clinical resistance. Clin Microbiol Rev. 1995;8:55784.PubMed
  20. Roszak DB, Colwell RR. Survival strategies of bacteria in the natural environment. Microbiol Rev. 1987;51:36579.PubMed
  21. Leff LG, Dana JR, McArthur JV, Shimkets LJ. Comparison of methods of DNA extraction from stream sediments. Appl Environ Microbiol. 1995;61:11413.PubMed


Suggested citation: Ash RJ, Mauck B and Morgan M. Antibiotic Resistance of Gram-Negative Bacteria in Rivers, United States. Emerg Infect Dis. [serial on the Internet]. 2002 Jul [date cited]. Available from

DOI: 10.3201/eid0807.010264

Table of Contents – Volume 8, Number 7—July 2002


Please use the form below to submit correspondence to the authors or contact them at the following address:

Ronald J. Ash, Department of Biology, Washburn University, Topeka, KS 66621, USA; fax: 785-231-1089;

character(s) remaining.

Comment submitted successfully, thank you for your feedback.