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Applied and Environmental Microbiology, August 2006, p. 5610-5614, Vol. 72, No. 8
0099-2240/06/$08.00+0     doi:10.1128/AEM.00364-06
Copyright © 2006, American Society for Microbiology. All Rights Reserved.

SHORT REPORT

Quantitative PCR Method for Sensitive Detection of Ruminant Fecal Pollution in Freshwater and Evaluation of This Method in Alpine Karstic Regions

Georg H. Reischer,1 David C. Kasper,1 Ralf Steinborn,2 Robert L. Mach,1 and Andreas H. Farnleitner1*

Institute for Chemical Engineering, Gene Technology Group, Vienna University of Technology, Getreidemarkt 9/166, A-1060 Vienna, Austria,1 Institute of Animal Breeding and Genetics, Department for Animal Breeding and Reproduction, University of Veterinary Medicine, Veterinaerplatz 1, A-1210 Vienna, Austria2

Received 14 February 2006/ Accepted 8 May 2006


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ABSTRACT
 
A quantitative TaqMan minor-groove binder real-time PCR assay was developed for the sensitive detection of a ruminant-specific genetic marker in fecal members of the phylum Bacteroidetes. The qualitative and quantitative detection limits determined were 6 and 20 marker copies per PCR, respectively. Tested ruminant feces contained an average of 4.1 x 109 marker equivalents per g, allowing the detection of 1.7 ng of feces per filter in fecal suspensions. The marker was detected in water samples from a karstic catchment area at levels matching a gradient from negligible to considerable ruminant fecal influence (from not detectable to 105 marker equivalents per liter).


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INTRODUCTION
 
Groundwater resources from alpine and mountainous karst aquifers play an important role in public water supplies throughout the world (15). Occasionally, karst springs show vulnerability to fecal contamination from point sources like leaking septic systems and nonpoint sources like wildlife and grazing livestock (29). The identification and apportioning of the sources of fecal contamination could make management and mitigation of this problem much easier and more cost-effective (28). Microbial source tracking (MST) serves this purpose and makes it possible to pinpoint pollution sources. Anaerobic bacteria of the phylum Bacteroidetes are highly abundant in feces (32), have been proposed as fecal indicator organisms (2, 3, 13), and exhibit host adaptation on the genetic level (10, 16). More recently, these bacteria became the target of MST efforts (20, 21). Bernhard and Field (4) identified source-specific genetic markers and developed methods for their qualitative detection, which were subsequently applied in practice (5, 6, 8) and improved (27). The aim of this study was to establish a method for the sensitive quantification of ruminant fecal pollution in spring water and groundwater from alpine karstic regions important for public water supplies.


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Sampling and DNA extraction of feces and water.
 
More than 300 fecal samples were collected in a large alpine catchment area in the Northern Calcareous Alps (area, 100 km2; latitude, 47°35'N to 47°43'N; longitude, 15° to 15°20'E; for a description of the study area, see reference 12) and to some extent from the larger area of eastern Austria. For pooled fecal samples, 10 single samples were combined and homogenized. Samples were collected in sterile fecal sampling tubes and stored at –20°C. DNA was extracted from 100 mg of each fecal sample using the Ultra Clean Soil DNA kit (MoBio Laboratories, Carlsbad, CA) in combination with bead beating (FastPrep FP120, Bio-101, Vista, CA; speed setting, 6 for 30 seconds). DNA was stored at –20°C. Water samples were collected in clean and autoclaved Nalgene (Nalge Europe, Hereford, United Kingdom) sampling bottles, stored in dark cooling boxes at 4°C during transport, and processed within 6 h after collection. A given volume of spring water was filtered through Isopore 0.2-µm polycarbonate membrane filters (Millipore, Bedford, MA). Three independent filtrations were done for each sample. Immediately after filtration, the filters were frozen and stored at –80°C until nucleic acid extraction. Nucleic acid extraction was performed as described by Griffiths et al. (17); samples were dissolved in 50 µl of sterile distilled water and stored at –80°C. All analyzed DNA extracts of fecal and aquatic origin contained amplifiable bacterial DNA as checked by applying a universal bacterial PCR assay (34).


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Assay development.
 
The following published 16S rRNA gene sequences were aligned with the Vector NTI software (InforMax, Oxford, United Kingdom): AF233400, AF233402, AF233403, and AF233404 (4) and AF294903, AF294904, AF294905, AF294906, AF294908, and AF294909 (5). Primers BacR_f and BacR_r (Table 1) were designed from the derived consensus sequence using Primer Express software (Applied Biosystems, Foster City, CA). The designed primers were used to amplify a 118-bp fragment from 10–2 dilutions of DNA extracts from ruminant fecal samples to obtain additional sequence information for quantitative PCR (qPCR) probe design. PCR was performed on an iCycler (Bio-Rad, Hercules, CA) using the following program: 95°C for 3 min; 30 cycles of 95°C for 15 s, 60°C for 15 s, and 72°C for 45 s; and 72°C for 3 min. Reaction mixtures (25 µl) contained 2.5 µl of sample DNA dilution, 200 nM BacR_f, 200 nM BacR_r, 10 µg bovine serum albumin (Boehringer Mannheim, Mannheim, Germany), and 12.5 µl of iQ Supermix (Bio-Rad). All PCR products were checked by agarose gel electrophoresis for correct size. PCR was performed from DNAs of two single and one pooled fecal sample each for cattle, deer, and chamois from representative locations in the study area. The PCR amplicons were then cloned into a pGEM-T vector (Promega, Madison, WI) and transformed into Escherichia coli JM 109. After purification of the plasmid DNA with the Quantum Prep Plasmid Miniprep Kit (Bio-Rad), the cloned inserts were sequenced by MWG-Biotech (Ebersberg, Germany). The sequences retrieved by cloning showed very high similarity, even between different ruminant sources (sequence identities above 74%). The TaqMan minor-groove binder probe BacR_p (Applied Biosystems) (Table 1) was designed using Primer Express. TaqMan minor-groove binder probes offer the additional advantage of being shorter and more specific than regular 5' nuclease probes (1, 22).


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  		TABLE 1. Primers and probe for the BacR qPCR assay developed in this study

qPCR was monitored on an iCycler iQ Real-Time Detection system. The optimized reaction mixture composition was 2.5 µl of sample DNA dilution, 100 nM BacR_f, 500 nM BacR_r, 100 nM BacR_p, 10 µg bovine serum albumin (Boehringer Mannheim), 12.5 µl of iQ Supermix (Bio-Rad), 2 mM additional MgCl2 (Bio-Rad), and water to a final volume of 25 µl. The PCR program was as follows: 95°C for 3 min and 50 cycles of 95°C for 15 s, 60°C for 15 s, and 72°C for 45 s. All reactions were performed in triplicate and in at least two 10-fold dilution steps. One of the specific clones (GenBank accession number DQ364808) was used for the generation of a plasmid standard-dilution series for qPCR detection. The concentration of the plasmid standard solution was measured photometrically. The standard was 10-fold serially diluted in a 5-ng/µl poly(dI-dC) solution as nonspecific DNA background (Roche Diagnostics, Mannheim, Germany). A total of six 10-fold serial dilutions of plasmid standard (5 to 5 x 105 gene copies) were run in triplicate on every well plate, as well as a no-template control and a no-amplification control (containing standard and 0.01% sodium dodecyl sulfate).


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Evaluation setup.
 
For the determination of the limit of detection in applied use, raw water from an alpine karst spring was filtered through a 0.22-µm Steritop membrane filter (Millipore). Three pooled fecal samples each (each consisting of 10 single samples) from cattle, deer, and chamois were analyzed in this experiment. One gram of wet feces from each sample was suspended in 50 ml of filtered spring water, and 100-fold dilution steps were prepared down to a concentration of 2 x 10–10 g wet feces per ml using the same water. One milliliter from each dilution step was filtered through 0.2-µm polycarbonate membrane filters (Millipore), the DNA was extracted, and qPCR was performed. Additionally, 100 and 500 ml of the spring water used for the suspensions were filtered and analyzed as negative controls.

To assess the occurrence of marker in the study area, samples were taken from the following water sources: spring KPAS (a well-protected spring site), spring LKAS2 (a relatively vulnerable karstic spring site; mean water residence time, 0.8 to 1.5 years; quick discharge response after precipitation; described in detail in reference 12), a river (a small river, influenced by several villages), a watering pond (situated in a fenced game-feeding compound), and a watering brook (running through a remote game-feeding compound). Sampling dates were as follows: KPAS, November 2005; LKAS2, June 2005; LKAS2 flood, August 2005 during a flood event; and river, watering pond, and watering brook, December 2005.


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Characteristics of the BacR qPCR assay.
 
Absolute quantification of the copy number of the ruminant-specific marker was achieved by analyzing a plasmid standard-dilution series with a known copy number in every measurement run. The marker copy number of any unknown sample could be determined from the respective standard regression curves (PCR efficiencies, >98% for all runs; R2 > 0.99). The qualitative detection limit was in the range of a few copies of the marker per reaction volume. Marker quantification was possible in the range from 20 to 107 marker copies per reaction volume. The presence of PCR inhibitors was assessed by analyzing DNA from water and fecal samples in 10-fold dilution steps. No inhibitory effects could be observed in any water samples, allowing the use of undiluted DNA extracts. For fecal samples, we tested 10 representative fecal-DNA extracts in four serial 10-fold dilutions. Inhibition was apparent in the undiluted DNA extract. In order to rule out any inhibition, we used 100-fold-diluted fecal-DNA extracts in the test of specificity.


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Source specificity.
 
The specificity of the assay was tested on DNA extracted from fecal samples from ruminant and nonruminant animals, as well as humans (Table 2). Among the group of ruminants, single samples were tested to measure the frequency of presence of the marker in ruminant fecal samples. For all other groups, the absence of the marker was demonstrated by analyzing pooled samples derived from 10 single samples whenever available. The prevalence of the marker among ruminants was 100%. Amplification was absent in all nonruminant sources (n = 146; 101 samples from nonruminant animals, 30 samples from human individuals, 13 samples from cesspits of alpine huts, and 2 samples of municipal wastewater from a small village in the study area) (Table 2).


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  		TABLE 2. Specificity of the BacR qPCR assay tested on ruminant and nonruminant animal fecal samples and human pooled fecal samples from cesspits and wastewater


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Limit of detection in applied use.
 
It was not possible to relate the copy numbers of our marker directly to a cell count of Bacteroidetes cells carrying this marker because the strain has not been isolated yet. We chose to express the results as marker equivalents detected in the PCR assay and assessed the number of those equivalents present in pooled ruminant feces suspended in water as the environmental matrix of interest. After filtration and DNA extraction, the marker equivalent concentration was determined, signifying the actual copy number of marker still detectable after the losses incurred in the preceding steps. Pooled samples were chosen in this experiment to reflect the average marker concentrations present in ruminant feces. Detection was possible in all nine pooled samples down to a filtered volume containing 2 x 10–8 g wet feces, while higher-dilution steps contained no detectable marker. The marker was present in ruminant feces at an average concentration of 4.1 x 109 marker equivalents per g wet feces. The values showed little variation, which is a consequence of the pooling process rather than being attributable to population dynamics (Table 3). From these results, we extrapolated the lowest detectable concentrations of ruminant feces. We tried to give a realistic estimate of the detectable marker equivalent concentration by assuming a Poisson distribution in the samples and defining a detection frequency of 95% (according to reference 23, the following formula applies: S = Xm ± {surd}Xm, where S is the 95% confidence interval and Xm is the average). Taking this into account, the reliable detection of the marker can only be expected in PCRs containing an average of six or more copies. The average detection limit of ruminant fecal material was 1.7 x 10–9 g per analyzed filter (Table 3).


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  		TABLE 3. Marker equivalent concentrations in suspended feces and detection limits in suspensions

qPCR has been demonstrated to be useful in the quantification of microorganisms in the environment (9, 18, 24, 25, 31, 33). The general applicability of probe-based qPCR in spring water was demonstrated by our group (30). Bernhard and Field (5) determined detection limits in the range from 2.8 x 10–5 to 2.8 x 10–7 g feces per liter using a qualitative PCR assay for their ruminant Bacteroides markers (approximately 100 times less sensitive than the BacR qPCR). In another publication, the detection limit of a qPCR assay for the detection of Rhodococcus coprophilus was 1 CFU per reaction (26). Since this bacterium is present at levels between 5.5 x 103 and 3.6 x 106 CFU per gram of herbivore feces, this method exhibits a sensitivity even lower than that of the above-mentioned conventional PCR assay for detection of Bacteroides marker (5). The high sensitivity of the BacR assay is also demonstrated by comparing it with cultivation-based fecal indicators. As an example, the concentrations of cultivable E. coli organisms in feces from cattle, deer, and chamois range from 4.0 x 106 to 7.7 x 107 CFU per g, with an average of 2 x 107 CFU per g (11) compared to the average of 4.1 x 109 marker equivalents per g measured in this study. This results in a 100-times-higher sensitivity with the BacR qPCR assay. On the other hand, the PCR method allows no assessment of the viability of fecal bacteria. Future investigation will have to establish correlations and differences between viability-based assays and direct-detection methods in the investigated environment.


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Occurrence of the marker throughout the study area.
 
To investigate the quantitative occurrence of the ruminant marker in the study area, water samples were taken from selected aquatic habitats covering a presumptive fecal-pollution gradient ranging from well-protected springs to heavily influenced surface waters. The marker could be found at concentrations ranging from not detectable in 4.5 liters (KPAS) to 106 marker equivalents per liter (LKAS2 flood) (Table 4). Strong differences in occurrence were obvious and in accordance with the expected different levels of ruminant fecal influence. The LKAS2 site showed low marker levels in early summer, when fecal indicators were not detectable, while the levels during a strong summer flood event were very high, corresponding to high fecal-indicator counts in the same sample (1.6 x 103 E. coli organisms per liter) (unpublished data). To our knowledge, no method with comparable performance for the specific detection of ruminant fecal contamination has been available up to now. In addition, the method is relatively fast and simple. In contrast, most established MST methods are either extremely laborious, like library-based typing methods (28), or not sensitive enough for spring water sources (26).


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  		TABLE 4. Levels of ruminant marker equivalent concentrations measured in samples taken throughout the study areaa


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Possible limitations of the assay.
 
For future applications, it will be necessary to estimate the persistence of the marker in the investigated environment as related to the hydrological situation. For the alpine karstic system, we performed preliminary experiments testing the stability of the marker in highly diluted fecal suspensions in spring water at ambient temperatures (4°C) and found no strong reduction of detectable marker levels during an incubation period of 2 months (data not shown). This result is in accordance with findings for human-specific Bacteroidetes markers (27). However, in aquatic systems with higher temperature and trophic status, an increased decay of the detectable marker can be expected. In addition, it will be necessary to investigate the occurrence of the marker in soils and sediments potentially influencing the water body of interest. It can be assumed that the source-specific organisms detected by this assay are highly adapted to the intestinal tracts of warm-blooded ruminant animals and are thus unlikely to proliferate in a soil habitat. Nevertheless, soil might be an intermittent storage reservoir for these bacteria.


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Potential applications.
 
The high sensitivity and specificity of the assay apparently meet the set requirement for the detection of fecal contamination in karstic spring water. After additional evaluation, the assay might allow the specific allocation of fecal pollution in alpine water sources, enabling target-oriented measures in the catchment area and thus facilitating watershed management (7, 19). Furthermore, it could also provide additional information for quantitative microbial risk assessment studies as part of water safety plans recommended by the WHO (35), allowing the relative estimation of ruminant fecal input compared to other sources. The current study was restricted to the areas of eastern Austria. The speculation of a cosmopolitan occurrence of the BacR marker is supported by studies from the United States, where fecal rRNA gene clones that exhibited sequences identical to those of the primer and probe binding sites of this assay were retrieved (5, 14). Evaluation in other regions will determine the method's general usefulness for scientists doing MST studies, as well as water suppliers trying to improve source water quality.


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Nucleotide sequence accession numbers.
 
Sequences are available at GenBank under accession numbers DQ364808 to DQ364822.


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ACKNOWLEDGMENTS
 
Our special thanks go to Hermann Kain for his unceasing enthusiasm and to all the tireless sample gatherers.


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FOOTNOTES
 
* Corresponding author. Mailing address: Institute for Chemical Engineering, Gene Technology Group, Vienna University of Technology, Getreidemarkt 9-166/5, A-1060 Vienna, Austria. Phone: 43-1-58801-17251. Fax: 43-1-5816266. E-mail: A.Farnleitner{at}aon.at. Back


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REFERENCES
 
    1
  1. Afonina, I., M. Zivarts, I. Kutyavin, E. Lukhtanov, H. Gamper, and R. B. Meyer. 1997. Efficient priming of PCR with short oligonucleotides conjugated to a minor groove binder. Nucleic Acids Res. 25:2657-2660.[Abstract/Free Full Text]
    2. 2
  2. Allsop, K., and D. J. Stickler. 1985. An assessment of Bacteroides fragilis group organisms as indicators of human faecal pollution. J. Appl. Bacteriol. 58:95-99.[Medline]
    3. 3
  3. Allsop, K., and D. J. Stickler. 1984. The enumeration of Bacteroides fragilis group organisms from sewage and natural waters. J. Appl. Bacteriol. 56:15-24.[Medline]
    4. 4
  4. Bernhard, A. E., and K. G. Field. 2000. Identification of nonpoint sources of fecal pollution in coastal waters by using host-specific 16S ribosomal DNA genetic markers from fecal anaerobes. Appl. Environ. Microbiol. 66:1587-1594.[Abstract/Free Full Text]
    5. 5
  5. Bernhard, A. E., and K. G. Field. 2000. A PCR assay to discriminate human and ruminant feces on the basis of host differences in Bacteroides-Prevotella genes encoding 16S rRNA. Appl. Environ. Microbiol. 66:4571-4574.[Abstract/Free Full Text]
    6. 6
  6. Bernhard, A. E., T. Goyard, M. T. Simonich, and K. G. Field. 2003. Application of a rapid method for identifying fecal pollution sources in a multi-use estuary. Water Res. 37:909-913.[Medline]
    7. 7
  7. Australian Federal Ministry of Agriculture, Forestry, Environment and Water, Management. 2001. Drinking water act, vol. 304. Government of Austria, Vienna, Austria.
    8. 8
  8. Boehm, A. B., J. A. Fuhrman, R. D. Mrse, and S. B. Grant. 2003. Tiered approach for identification of a human fecal pollution source at a recreational beach: case study at Avalon Bay, Catalina Island, California. Environ. Sci. Technol. 37:673-680.[Medline]
    9. 9
  9. Brinkman, N. E., R. A. Haugland, L. J. Wymer, M. Byappanahalli, R. L. Whitman, and S. J. Vesper. 2003. Evaluation of a rapid, quantitative real-time PCR method for enumeration of pathogenic Candida cells in water. Appl. Environ. Microbiol. 69:1775-1782.[Abstract/Free Full Text]
    10. 10
  10. Dick, L. K., A. E. Bernhard, T. J. Brodeur, J. W. Santo Domingo, J. M. Simpson, S. P. Walters, and K. G. Field. 2005. Host distributions of uncultivated fecal Bacteroidales bacteria reveal genetic markers for fecal source identification. Appl. Environ. Microbiol. 71:3184-3191.[Abstract/Free Full Text]
    11. 11
  11. Farnleitner, A. H., R. L. Mach, M. M. Burtscher, G. H. Reischer, G. Ryzinska, K. Keiblinger, S. Rudnicki, S. Knetsch, and R. Sommer. 2005. "Back to the roots"—incidence and abundance of faecal indicators in faeces and sewage of potential pollution sources in an alpine karstic catchment area, abstr. 13. 13th Int. Symp. Health-Related Microbial. International Water Association, Swansea, Wales.
    12. 12
  12. Farnleitner, A. H., I. Wilhartitz, G. Ryzinska, A. K. Kirschner, H. Stadler, M. M. Burtscher, R. Hornek, U. Szewzyk, G. Herndl, and R. L. Mach. 2005. Bacterial dynamics in spring water of alpine karst aquifers indicates the presence of stable autochthonous microbial endokarst communities. Environ. Microbiol. 7:1248-1259.[CrossRef][Medline]
    13. 13
  13. Fiksdal, L., J. S. Maki, S. J. LaCroix, and J. T. Staley. 1985. Survival and detection of Bacteroides spp., prospective indicator bacteria. Appl. Environ. Microbiol. 49:148-150.[Abstract/Free Full Text]
    14. 14
  14. Fogarty, L. R., and M. A. Voytek. 2005. Comparison of bacteroides-prevotella 16S rRNA genetic markers for fecal samples from different animal species. Appl. Environ. Microbiol. 71:5999-6007.[Abstract/Free Full Text]
    15. 15
  15. Ford, D. C., and P. W. Williams. 1996. Karst geomorphology and hydrology. Chapman & Hall, London, United Kingdom.
    16. 16
  16. Gordon, D. M. 2001. Geographical structure and host specificity in bacteria and the implications for tracing the source of coliform contamination. Microbiology 147:1079-1085.[Free Full Text]
    17. 17
  17. Griffiths, R. I., A. S. Whiteley, A. G. O'Donnell, and M. J. Bailey. 2000. Rapid method for coextraction of DNA and RNA from natural environments for analysis of ribosomal DNA- and rRNA-based microbial community composition. Appl. Environ. Microbiol. 66:5488-5491.[Abstract/Free Full Text]
    18. 18
  18. Guy, R. A., P. Payment, U. J. Krull, and P. A. Horgen. 2003. Real-time PCR for quantification of Giardia and Cryptosporidium in environmental water samples and sewage. Appl. Environ. Microbiol. 69:5178-5185.[Abstract/Free Full Text]
    19. 19
  19. Kralik, M. 2001. Strategie zum Schutz der Karstwassergebiete in Österreich, vol. BE-189. Austrian Environmental Protection Agency, Vienna, Austria.
    20. 20
  20. Kreader, C. A. 1995. Design and evaluation of Bacteroides DNA probes for the specific detection of human fecal pollution. Appl. Environ. Microbiol. 61:1171-1179.[Abstract]
    21. 21
  21. Kreader, C. A. 1998. Persistence of PCR-detectable Bacteroides distasonis from human feces in river water. Appl. Environ. Microbiol. 64:4103-4105.[Abstract/Free Full Text]
    22. 22
  22. Kutyavin, I. V., I. A. Afonina, A. Mills, V. V. Gorn, E. A. Lukhtanov, E. S. Belousov, M. J. Singer, D. K. Walburger, S. G. Lokhov, A. A. Gall, R. Dempcy, M. W. Reed, R. B. Meyer, and J. Hedgpeth. 2000. 3'-minor groove binder-DNA probes increase sequence specificity at PCR extension temperatures. Nucleic Acids Res. 28:655-661.[Abstract/Free Full Text]
    23. 23
  23. Lorenz, R. J. 1992. Grundbegriffe der Biometrie. Gustav Fischer Verlag Stuttgart, Jena, Germany.
    24. 24
  24. Reischer, G. H., M. Lemmens, A. Farnleitner, A. Adler, and R. L. Mach. 2004. Quantification of Fusarium graminearum in infected wheat by species specific real-time PCR applying a TaqMan probe. J. Microbiol. Methods 59:141-146.[CrossRef][Medline]
    25. 25
  25. Roe, J. D., R. A. Haugland, S. J. Vesper, and L. J. Wymer. 2001. Quantification of Stachybotrys chartarum conidia in indoor dust using real time, fluorescent probe-based detection of PCR products. J. Exp. Anal. Environ. Epidemiol. 11:12-20.[CrossRef][Medline]
    26. 26
  26. Savill, M. G., S. R. Murray, P. Scholes, E. W. Maas, R. E. McCormick, E. B. Moore, and B. J. Gilpin. 2001. Application of polymerase chain reaction (PCR) and TaqMan PCR techniques to the detection and identification of Rhodococcus coprophilus in faecal samples. J. Microbiol. Methods 47:355-368.[CrossRef][Medline]
    27. 27
  27. Seurinck, S., T. Defoirdt, W. Verstraete, and S. D. Siciliano. 2005. Detection and quantification of the human-specific HF183 Bacteroides 16S rRNA genetic marker with real-time PCR for assessment of human faecal pollution in freshwater. Environ. Microbiol. 7:249-259.[CrossRef][Medline]
    28. 28
  28. Simpson, J. M., J. W. Santo Domingo, and D. J. Reasoner. 2002. Microbial source tracking: state of the science. Environ. Sci. Technol. 36:5279-5288.[Medline]
    29. 29
  29. Sinton, L. W., R. K. Finlay, and D. J. Hannah. 1998. Distinguishing human from animal faecal contamination in water: a review. N. Z. J. Mar. Freshwater Res. 32:323-348.
    30. 30
  30. Stricker, A. R., I. Wilhartitz, A. H. Farnleitner, and R. L. Mach. 30 May 2006, posting date. Development of a Scorpion probe based real-time PCR for the sensitive quantification of Bacteroides sp. ribosomal DNA from human and cattle origin and evaluation in spring water matrices. Microbiol. Res. [Online.] http://www.elsevier.de/artikel/805099&_text=toc&_text=&_text=beschreiburg.
    31. 31
  31. Stults, J. R., O. Snoeyenbos-West, B. Methe, D. R. Lovley, and D. P. Chandler. 2001. Application of the 5' fluorogenic exonuclease assay (TaqMan) for quantitative ribosomal DNA and rRNA analysis in sediments. Appl. Environ. Microbiol. 67:2781-2789.[Abstract/Free Full Text]
    32. 32
  32. Suau, A., R. Bonnet, M. Sutren, J. J. Godon, G. R. Gibson, M. D. Collins, and J. Dore. 1999. Direct analysis of genes encoding 16S rRNA from complex communities reveals many novel molecular species within the human gut. Appl. Environ. Microbiol. 65:4799-4807.[Abstract/Free Full Text]
    33. 33
  33. Suzuki, M. T., L. T. Taylor, and E. F. DeLong. 2000. Quantitative analysis of small-subunit rRNA genes in mixed microbial populations via 5'-nuclease assays. Appl. Environ. Microbiol. 66:4605-4614.[Abstract/Free Full Text]
    34. 34
  34. Teske, A., C. Wawer, G. Muyzer, and N. B. Ramsing. 1996. Distribution of sulfate-reducing bacteria in a stratified fjord (Mariager Fjord, Denmark) as evaluated by most-probable-number counts and denaturing gradient gel electrophoresis of PCR-amplified ribosomal DNA fragments. Appl. Environ. Microbiol. 62:1405-1415.[Abstract]
    35. 35
  35. WHO. 2004. Guidelines for drinking-water quality, 3rd ed. World Health Organization, Geneva, Switzerland.

Applied and Environmental Microbiology, August 2006, p. 5610-5614, Vol. 72, No. 8
0099-2240/06/$08.00+0     doi:10.1128/AEM.00364-06
Copyright © 2006, American Society for Microbiology. All Rights Reserved.



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