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Applied and Environmental Microbiology, July 1999, p. 3142-3147, Vol. 65, No. 7
Department of Family,
Received 19 February 1999/Accepted 26 April 1999
Estuarine waters receive fecal pollution from a variety of sources,
including humans and wildlife. Escherichia coli is a
ubiquitous bacterium in the intestines of warm-blooded animals and is
used as an indicator of fecal pollution. However, its presence does not
specifically differentiate sources of pollution. A total of 238 E. coli isolates from human sources (HS) and nonhuman
sources (NHS) were collected from the Apalachicola National Estuarine Research Reserve, from associated sewage treatment plants, and directly
from animals and tested for ribotype (RT) profile. HS and NHS isolates
showed 41 and 61 RT profiles, respectively. At a similarity index
of ca. 50%, HS and NHS isolates demonstrated four clusters, with the
majority of HS and NHS isolates located in clusters C and D; isolates
obtained directly from human and animal feces also could be grouped
within these clusters. Discriminant analysis (DA) of RT profiles showed
that 97% of the NHS isolates and 100% of the animal fecal isolates
were correctly classified. The average rate of correct classification
for HS and NHS isolates was 82%. We conclude that DA of RT profiles
may be a useful method for identifying HS and NHS fecal pollution and
may potentially facilitate management practices.
Fecal pollution is a major concern
for many estuaries, where it can originate from human sources
(HS) and nonhuman sources (NHS). Its impact can degrade water quality
and restrict its use for harvesting sea foods, as well as recreational
activities. However, without knowing the precise source of fecal
input, the human health risk cannot be accurately predicted.
The fecal coliform Escherichia coli has been used as an
indicator of human enteric pathogens for many years (12).
However, it is now well established that E. coli is not
limited to humans but also exists in the intestines of many other
warm-blooded animals (22). Consequently, its presence in
water is not specific to human sources of pollution.
This is especially relevant when recognizing that human feces can
carry various human enteric pathogens, such as
Salmonella spp., Shigella spp., E. coli, hepatitis A virus, and Norwalk group viruses. In contrast,
most of these pathogens do not colonize nonhuman species, potentially
resulting in less risk posed by NHS fecal pollution (16, 17, 22,
32). Therefore, it is important to know whether fecal
pollution originates from HS or NHS in order to properly assess risk,
and research is needed to determine the characteristics of indicators,
such as E. coli, that may be used to identify sources of pollution.
To meet this challenge, there have been various attempts to develop
methods that differentiate the sources of fecal
pollution. Initially, the ratio of fecal coliforms to
fecal streptococci was proposed, where a ratio of Investigators have also reported that nonhuman and human feces contains
different serotypes of RNA coliphages (11, 22), suggesting
that phages could be used to predict the source of pollution.
However, their usefulness is limited, because only a small percentage
of human fecal samples contain phages (22).
More-traditional methods for discriminating bacteria have included
biochemical tests (1, 21), phage susceptibility
(38), outer membrane protein profiles (8),
antibody reactivity (36), fimbriation (18),
bacteriocin production and susceptibility, and other methods
(14). However, these systems have serious disadvantages,
including unstable phenotypes, low sensitivity at the intraspecies
level, and limited specificity (33). Even with these
limitations, we have recently reported that multiple antibiotic
resistance (MAR) can be used to differentiate point and nonpoint
sources of E. coli in an estuarine environment
(25).
Some of the more recent techniques involve DNA analysis, such as
plasmid profiles, pulsed-field gel electrophoresis (6, 23),
and restriction fragment length polymorphism analysis at specific loci,
such as fimbrial adhesion and rRNA (ribotyping) operons (15,
18). These methods are generally less dependent on the more
unstable phenotypic traits.
Ribotyping has proved to be a useful epidemiological technique for
various bacteria, including E. coli (33),
Salmonella enterica (21), Vibrio
cholerae O1 (27), and Vibrio vulnificus (7, 34). However, an examination of the literature shows that this method has not been used to discriminate HS and NHS E. coli strains.
Any new predictive test requires extensive statistical modeling of the
data to correlate specific bacterial characteristics with their source.
Discriminant analysis (DA) can classify individuals into groups on the
basis of several classification variables (5).
To test the applicability of ribotyping to predict the source of
E. coli pollution, we selected the Apalachicola National Estuarine Research Reserve (ANERR), a site where we have previously studied MAR in over 700 E. coli isolates (25).
The ANERR consists of two barrier islands, the lower 20 miles of the
Apalachicola River and its flood plain, adjoining uplands, and the
Apalachicola Bay system (10, 25). The ANERR is also a
significant harvest area for shellfish and a variety of finfish
(10). We found that DA of E. coli ribotype (RT)
profiles predicted the source of E. coli pollution.
E. coli isolates.
E. coli isolates were
selected from among 700 isolates previously described in an earlier
study of MAR (25). For the present RT studies, 179 isolates
were selected in proportion to the number of isolates in specific MAR
clusters; an additional 30 and 29 isolates were directly isolated from
human and wildlife feces, respectively (25). E. coli was isolated and identified by standard procedures (3,
4, 25).
RT analyses.
For RT analyses, E. coli ATCC 9637 was used as the control strain.
(i) DNA extraction.
DNA was extracted by the method of
Sambrook et al. (29). Briefly, E. coli were grown
in brain heart infusion broth (Difco Laboratories, Detroit, Mich.), and
late-log-phase cultures were pelleted at 3,000 × g for
15 min and treated with lysozyme (10 mg/ml; Sigma), proteinase K (10 mg/ml; Fisher Biotech, Fair Lawn, N.J.), and RNase (150 µg/ml;
Fisher) at 37°C for 30 min. DNA was extracted with chloroform-isoamyl
alcohol (24:1), precipitated with 100% isopropanol, washed once in
70% ethanol, recovered, dried, and resuspended in TE buffer (10 mM
Tris-HCl, 1 mM EDTA; pH 8.0).
(ii) Determination of DNA concentration.
DNA concentration
was determined by using a TKO 100 Mini-Fluorometer according to the
manufacturer's instructions (Hoefer Scientific Instruments, San
Francisco, Calif.). Two microliters of a 100-µg/ml concentration of
calf thymus DNA was used as a standard.
(iii) Restriction enzyme analysis.
Approximately 1 µg of
DNA was digested with several restriction enzymes, including
HindIII, EcoRI, SalI, and
BglI (Gibco BRL, Gaithersburg, Md.), according to the
manufacturer's instructions. Digested DNA was separated in a 1.0%
agarose gel at 30 V for 16 h in TBE buffer (0.09 M Tris-borate,
0.002 M EDTA), stained with ethidium bromide (5 µg/ml), and
photographed under shortwave UV light. A HindIII digest
of bacteriophage lambda (Promega Corp., Madison, Wis.) was used as a
molecular weight marker.
(iv) Southern blot analysis.
After electrophoresis of
restriction-digested DNA, agarose gels were denatured in 0.5 M
NaOH-1.5 M NaCl for 35 min and neutralized in 0.5 M Tris-HCl (pH
7.2)-1.5 M NaCl-0.001 M disodium EDTA for 45 min. DNA was then
blotted from gels onto nylon membranes (Bio-Rad Laboratories, Hercules,
Calif.) by using a vacuum blotting system (VacuGene XL; Pharmacia
Biotech, Piscataway, N.J.) and fixed with shortwave UV light for 5 min
(31).
(v) Probe preparation.
E. coli 16S and 23S rRNA were
reverse transcribed into cDNA with avian reverse transcriptase
(Boehringer Mannheim Corp., Indianapolis, Ind.) and then labeled with
digoxigenin-dUTP according to the manufacturer's instructions
(Boehringer Mannheim Corp.).
(vi) Hybridization and detection.
Membranes were
prehybridized at 42°C for 2 h and then hybridized with a
digoxigenin-labeled probe with 25 ng of DNA per 15- by 15-cm filter at
65°C for 16 h. After hybridization, membranes were washed twice
for 5 min each time with 2× SSC (2× SSC is 0.3 M NaCl plus 30 mM
sodium citrate)-0.1% sodium dodecyl sulfate (SDS) at room temperature
and twice for 15 min each time with 0.5× SSC-0.1% SDS at 65°C;
membranes were then reacted with antibody and visualized by using
nitroblue tetrazolium and 5-bromo-4-chloro-3-indolyl-phosphate for
colorimetric detection according to the manufacturer's instructions (Boehringer Mannheim Corp.).
Statistical analysis.
RT profiles were measured by using DNA
Proscan software (Nashville, Tenn.). DNA fragments for each strain were
translated into binary code. Similarity indices were determined by
using Dice's coincidence index (9), where restriction
endonuclease digestion profile similarities
(Sxy) for individuals x and
y equals the numbers of common fragments in their DNA
profiles (nxy) divided by the average number of
fragments exhibited by both individuals (Sxy = 2nxy/nx + ny).
Relationships among isolates were examined by using cluster analysis.
Data management and cluster analysis were performed in SAS (SAS
Institute, Inc., Cary, N.C.), and cluster dendrograms were plotted by
using S-Plus software (Statistical Services, Inc., Seattle, Wash.).
Binary codes were also analyzed by using statistical discrimination
methodology (5, 19, 20), as implemented in SAS (SAS 1989 AIX, version 6.12). A test for homogeneity of within-group covariance
matrices suggested an unpooled covariance analysis, resulting in the
use of quadratic discriminant function. In addition, equal prior
probabilities were assumed. Results of the discrimination model were
summarized by use of the average rate of correct classification (ARCC)
and the percentage of correctly and misclassified isolates from the
classification table. The table is a source-by-source matrix in which
the numbers and percentages of correctly classified isolates were found
on the diagonal. The ARCC was computed by averaging the percentages along the diagonal of the table (the correctly classified isolates).
We analyzed RT profiles of 238 E. coli isolates (84 HS,
95 NHS, 30 human feces, and 29 animal feces). Preliminary
experiments examined several restriction enzymes
(HindIII, EcoRI, SalI, and BglI) with a panel of E. coli isolates to
determine the appropriate enzyme for this study. Results showed that
HindIII gave the most discriminating profile, consisting
of 4 to 12 bands over a size range of 0.7 to 20.0 kb, and thus it was
used for subsequent studies. Patterns were considered to be unique when
differentiated by one or more bands.
HS isolates showed 41 unique RT profiles, with more than 60% belonging
to 11 RTs (Fig. 1). A binary metric
average linkage plot of HS isolates at a similarity index of ca. 50%
demonstrated three clusters, designated RP1, RP2, and RP3; two isolates
(i.e., SPS 1 and SPS 603) were located outside of these clusters (Fig. 1). An even higher degree of homology was observed for HS isolates at a
more stringent level of similarity (Fig. 1 and
2). In contrast, NHS isolates exhibited
61 different RT profiles, with 14 RTs accounting for 50% of the
isolates (Fig. 2). A binary metric average linkage plot of NHS isolates
at the 50% similarity index showed five clusters, designated
RN1, RN2, RN3, RN4, and RN5; three isolates (i.e., SP 52, SP 69, and SP 444) were located outside of the clusters (Fig. 2).
We combined individual databases for HS and NHS isolates, and at a
similarity index of ca. 50% four clusters were obtained. The majority
of the HS and NHS isolates were located in clusters C and D. There were
24 unique RT patterns that contained more than one isolate and included
64 and 50% of the HS and NHS isolates, respectively. Eight patterns
contained only HS isolates, and another eight contained only NHS
isolates; the remaining patterns contained both HS and NHS isolates
(Table 1).
0099-2240/99/$04.00+0
Copyright © 1999, American Society for Microbiology. All rights reserved.
Discriminant Analysis of Ribotype Profiles of Escherichia
coli for Differentiating Human and Nonhuman Sources of
Fecal Pollution
ABSTRACT
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
INTRODUCTION
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
4.0 would indicate
HS pollution, whereas a ratio of 
0.7 would indicate NHS pollution
(13). However, this approach was unreliable due to the
variable survival rates of fecal streptococcus species (28).
MATERIALS AND METHODS
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
RESULTS
Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
View larger version (27K):
[in a new window]
FIG. 1.
Binary metric plot of average similarity linkage for RT
profiles of HS isolates digested with HindIII. The
prefix "SPS" indicates HS isolates. The similarity index is
indicated on the left axis.
View larger version (30K):
[in a new window]
FIG. 2.
Binary metric plot of average similarity linkage for RT
profiles of NHS isolates digested with HindIII. The
prefix "SP" indicates NHS isolates. The similarity index is
indicated on the left axis.
TABLE 1.
HS, NHS, human fecal, and animal fecal isolates at
different similarity indices
Ten E. coli isolates were obtained from each of three separate human fecal samples and then tested for RT. Different individuals showed different RT profiles. However, all of these human isolates were grouped within previously defined HS RT profiles (Table 1).
In addition, there were approximately five E. coli isolates obtained from five separate raccoons, as well as five isolates from wildlife of unknown origin. The RT patterns of raccoon isolates varied from raccoon to raccoon but demonstrated high homology (i.e., 93%) within the previously defined NHS clusters (Table 1). When animal fecal isolates were grouped in a cluster that contained both HS and NHS isolates, in most instances animal fecal isolates (e.g., C3) showed 100% similarity with NHS isolates.
DA of RT profiles showed that the ARCC was 82%. A total of 97 and 67% of the NHS and HS isolates, respectively, were correctly classified by the RT method.
DA of E. coli isolates obtained directly from human and animal feces showed that 67 and 100% of human and animal fecal isolates, respectively, were correctly classified; the ARCC was 84%.
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DISCUSSION |
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Top
Abstract
Introduction
Materials and Methods
Results
Discussion
References
|
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Techniques such as restriction endonuclease analysis (REA) of chromosomal DNA (i.e., DNA fingerprinting) and ribotyping (2, 30, 33) provide genotypic characteristics of bacteria that avoid the potential pitfalls associated with phenotypic methods. REA of chromosomal DNA is useful for the identification of many phenotypically indistinguishable bacteria (36). However, REA of E. coli produces many fragments, making visual comparisons of isolates difficult (data not shown). In contrast, RT yields patterns that allow much simpler comparisons among isolates (33). A major advantage of RT is that rRNA sequences are highly conserved and are present as multiple copies in bacterial genomes (15). Furthermore, one of the major benefits of RT is that 16S and 23S rRNA are commercially available.
In this study, ribotyping was used to discriminate HS and NHS E. coli isolates in a way similar to the way other investigators have used ribotyping to discriminate E. coli from different sources (24, 33, 35). From our study, we found that HS E. coli showed much less diversity than NHS isolates (Fig. 1 and 2). The latter situation may result from E. coli clones maintained in diverse reservoirs within the ANERR, such as raccoons, birds, deer, and other wildlife.
We also found that the HS and NHS clusters produced by the combined databases (Table 1) were in agreement with the RT profiles of isolates obtained directly from humans and wildlife. This finding strongly indicates that HS and NHS isolates may be derived from humans and raccoons and from unknown animal feces, respectively. Previously, we reported that MAR profiles of HS E. coli isolates showed greater resistance to antibiotics and higher MAR indices than those of NHS isolates. E. coli isolates obtained directly from human and animal feces could also be clustered by MAR among the HS and NHS isolates, respectively (25).
This study strongly indicates that DA of RT profiles can be used to differentiate HS and NHS of fecal pollution. Although some of the isolates were classified incorrectly, many more isolates were correctly classified than would be if the classification was random. This analysis also showed an ARCC well above that expected by chance (P < 0.05).
The advantage of DA is that it generates a classification rule based on all of the isolates; that rule can then be used to classify each individual isolate into one of many possible sources. Once a DA classification rule is developed by using RT profiles of E. coli isolates from known sources, DA can then be used to classify an unknown isolate to one of the known sources by using the unknown organism's RT profiles.
Wiggins (37) demonstrated that DA of antibiotic resistance patterns of fecal streptococci is a useful tool for differentiating human and animal sources of fecal pollution in water. He found that 92% of HS isolates could be classified with an ARCC of 84%. We have reported that DA of MAR profiles of E. coli isolates from the ANERR classified 82 and 68% of HS and NHS isolates, respectively, and that the ARCC was 75% (26). However, this method has certain disadvantages: the antibiotic resistance patterns of bacteria are influenced by selective pressure and thus may be different in other geographical areas and may vary over time. In contrast, RT profiles are a genetic characteristic and are not as easily influenced by selective pressure. Therefore, on the basis of these data, DA of RT profiles provides a strong method for differentiating HS and NHS fecal pollution and may enhance efforts to improve the natural and commercial quality of estuarine ecosystems and to assess the importance of upstream activities, local storm water runoff, and marine activities.
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ACKNOWLEDGMENTS |
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This research was supported by the U.S. Department of Commerce, National Oceanographic and Atmospheric Administration, Sanctuaries and Reserves Division (grant NA370R0166).
We are grateful to Leslie Miller, Tammi Stowers, and Mary McGinley for technical assistance. We thank Chip Bailey for assistance with sample collection.
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FOOTNOTES |
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* Corresponding author. Mailing address: P.O. Box 110287, University of Florida, Gainesville, FL 32611-0287. Phone: (352) 392-1885. Fax: (352) 846-1102. E-mail: mlt{at}gnv.ifas.ufl.edu.
Florida Agricultural Experiment Station journal series
no. R-06879.
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Results
Discussion
References
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Applied and Environmental Microbiology, July 1999, p. 3142-3147, Vol. 65, No. 7
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Copyright © 1999, American Society for Microbiology. All rights reserved.
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