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Applied and Environmental Microbiology, July 2004, p. 4035-4039, Vol. 70, No. 7
0099-2240/04/$08.00+0     DOI: 10.1128/AEM.70.7.4035-4039.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.

Evaluation of a Strategy for Toxoplasma gondii Oocyst Detection in Water

Isabelle Villena,^1,2* Dominique Aubert,^1,2 Philippe Gomis,² Hubert Ferté,^1,2 Jean-Christophe Inglard,³ Hélène Denis-Bisiaux,³ Julie-Muriel Dondon,⁴ Eric Pisano,^1,2 Naïma Ortis,^1,2 and Jean-Michel Pinon^1,2

Laboratoire de Parasitologie-Mycologie, CHU Maison Blanche, UFR Médecine,¹ EA 2070, IFR 53, Université de Reims Champagne-Ardenne, 51092 Reims,² Communauté de Communes de I'Agglomération de Reims (CCAR), 51096 Reims,³ Direction Régionale des Affaires Sanitaires et Sociales, Service Santé Environnement, 51037 ChÂlons en Champagne, France⁴

Received 8 October 2003/ Accepted 6 April 2004

Top Abstract Introduction Materials and Methods Results Discussion References

 
Several recent outbreaks of toxoplasmosis were related to drinking water. We propose a strategy for Toxoplasma oocyst detection as part of an approach to detecting multiple waterborne parasites, including Giardia and Cryptosporidium spp., by the U.S. Environmental Protection Agency method with the same sample. Water samples are filtered to recover Toxoplasma oocysts and purified on a sucrose density gradient. Detection is based on PCR and mouse inoculation (bioassay) to determine the presence and infectivity of recovered oocysts. In an experimental seeding assay with 100 liters of deionized water, a parasite density of 1 oocyst/liter was successfully detected by PCR in 60% of cases and a density of 10 oocysts/liter was detected in 100% of cases. The sensitivity of the PCR assay varied from less than 10 to more than 1000 oocysts/liter, depending on the sample source. PCR was always more sensitive than mouse inoculation. This detection strategy was then applied to 139 environmental water samples collected over a 20-month period. Fifty-three samples contained PCR inhibitors, which were overcome in 39 cases by bovine serum albumin addition. Among 125 interpretable samples, we detected Toxoplasma DNA in 10 cases (8%). None of the samples were positive by mouse inoculation. This strategy efficiently detects Toxoplasma oocysts in water and may be suitable as a public health sentinel method.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Toxoplasma gondii is a protozoan parasite capable of infecting a variety of birds and mammals, including humans (40). Toxoplasmosis is a significant problem in congenitally infected infants and immunosuppressed patients. T. gondii is transmitted in three main ways: (i) from mother to fetus, (ii) by consumption of undercooked meat containing tissue cysts, and (iii) by ingestion of food or water contaminated by sporulated oocysts. Members of the Felidae are the only known hosts that can release oocysts into the environment in their feces (11). Excreted oocysts are unsporulated and are not directly infectious. They become infective after 1 to 21 days in the external environment, depending on aeration and temperature (9). Although cats excrete oocysts over only short periods (1 to 3 weeks), they release massive numbers of oocysts (10⁷/10⁸), which are highly resistant and can survive for months in the environment (13).

Three waterborne toxoplasmosis outbreaks have been documented (2-4). The first occurred in Panama in 1979 (3). An epidemiological investigation identified the source as creek water contaminated by oocysts excreted by jungle cats. A large waterborne outbreak occurred in British Columbia (Canada) in 1995, with 110 cases of human acute Toxoplasma infection (4). The source was municipal drinking water, probably contaminated by cougar and/or domestic cat feces (1). The largest outbreak, with 290 human cases, was recently reported in Brazil and involved an unfiltered water reservoir (22). Bahia-Oliveira et al. found a high T. gondii prevalence in a Brazilian community, related to drinking unfiltered water (2). Likewise, Hall et al. identified drinking water as the probable source of infection in a community of strict vegetarians (18).

Waterborne transmission of the intestinal parasites Giardia duodenalis and Cryptosporidium parvum is also well documented (16, 36, 37). Over 160 waterborne outbreaks of giardiasis and cryptosporidiosis have been reported, and well-documented cases have been described in the United States and United Kingdom (26, 27, 29). T. gondii oocysts are resistant to the usual processes used to disinfect drinking water (42). Increase awareness of the risk of waterborne toxoplasmosis outbreaks has led to a search for methods that can efficiently detect oocysts in environmental water.

Here, we evaluated a strategy used since 2001 in our laboratory to detect T. gondii oocysts in water, along with Giardia spp. and Cryptosporidium spp. The strategy involves three basic steps: (i) concentration and filtration of the water sample to recover small numbers of Toxoplasma oocysts, (ii) elution and purification on a density gradient, and (iii) detection by PCR amplification and bioassay (mouse inoculation) to determine the presence and the infectivity of recovered oocysts. This strategy was applied to 139 water samples over a 20-month period.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Oocyst stock preparation.
Oocysts were isolated from the feces of a cat experimentally infected with 3,000 cysts of a chronic type II strain (RMS/99/GUI). Nonsporulated T. gondii oocysts were purified and induced to sporulate as described by Dubey and Frenkel (10). Briefly, in step 1, the feces were emulsified in water and centrifuged; the supernatant was discarded, and sediment 1 was recovered. Step 2 consisted of mixing sediment 1 with 10 volumes of sucrose solution (specific gravity, 1.15) and centrifuging (1,250 x g). After step 2, oocysts were found in supernatant 2. In step 3, approximately 5 ml of supernatant 2 was mixed with 45 ml of water and then centrifuged (1,250 x g); the oocysts were now in sediment 3. Five milliliters of 2% aqueous H₂SO₄ was added to sediment 3, and the tube was aerated at room temperature for 7 days. Sporulated oocysts were stored at 4°C until used in seeding experiments.

Seeding.
Samples of deionized water (DW), public drinking water (PDW), and raw surface water (RSW) (100 liters each) were seeded with known numbers of oocysts. The oocyst stock suspension was counted with a hemocytometer, and the mean value obtained for 10 different samples was analyzed. The stock suspension was adjusted to 10⁵ oocysts/ml. DW and PDW (100 liters) were seeded with 10² or 10³ oocysts, and RSW (40 liters; maximal filtration capacity) was seeded with 4 x 10⁴, 4 x 10³, or 4 x 10² oocysts.

Environmental samples.
The sampling sites were selected by local public health officials in the four departments of the Champagne-Ardenne region. The survey was carried out over a 20-month period (June 2001 to January 2003). A total of 139 samples were analyzed, consisting of RSW collected near water plant intakes (n = 45), underground water (UW) (n = 50), and PDW (n = 44). Samples from different geographical locations exhibited a range of turbidities measured by the nephelometric procedure; 100 liters was collected in 10-liter polypropylene barrels at each source and transported to the laboratory for immediate processing. The filtered volumes were 100 liters of PDW, 25 to 100 liters of UW, and 7 to 45 liters of RSW. Some samples also contained Giardia spp. and Cryptosporidium spp., which were detected by indirect immunofluorescence after immunomagnetic separation (IMS), using method 1623 of the U.S. Environmental Protection Agency (USEPA) (15).

Oocyst detection. (i) Filtration.
Each sample was concentrated using Envirochek capsules (Pall Gelman Laboratory) as specified by the manufacturer. We tested both the original Gelman Envirochek Standard (GES) (a polyethersulfonate membrane with a 1-µm absolute pore size, designed for 10 to 100-liter volumes) and Envirochek HV (GEHV) (a new 1-µm track-etched membrane for water volumes of 500 liters or more). All the samples were concentrated using GES capsules, and some (seeded DW) were also concentrated with GEHV capsules. Particulate matter was eluted from the capsule filter with elution buffer containing detergents (Tween 80 and Laureht-12; Pall Gelman Laboratory). Eluates were centrifuged (30 min at 1,250 x g and 4°C); distilled water was added to the pellet-eluting solution (adjusted to 10 ml), and the solution was subjected to IMS for detection of Giardia spp. and Cryptosporidium spp. After this IMS step, the eluate was centrifuged (10 min at 1,250 x g and 4°C), supernatant 1 was discarded and pellet 1 was suspended in sucrose suspension (density, 1.15; ratio: 1:3). After centrifugation (10 min at 1,250 x g and 4°C), 2 ml of supernatant 2 (which would contain oocysts) was collected and mixed with 8 ml of DW. After last centrifugation (10 min at 1,250 x g and 4°C), supernatant 3 was discarded and sediment 3 was used for T. gondii detection.

(ii) Detection.
The sediment obtained after sucrose separation was separated into two parts. One was used for PCR, and the other was used for bioassay (mouse inoculation) after sporulation.

(a) PCR detection.
The sediment was resuspended in 1 ml of Tris-EDTA buffer and centrifuged (3 min at 1,250 x g). Three cycles of freezing (–80°C)-thawing were done, and the pellet was subjected first to proteinase K digestion (1 h at 60°C) and then to DNA extraction with QIAamp DNA minikits (Qiagen, Courtaboeuf, France) as specified by the manufacturer. DNA was then subjected to real-time PCR for detection of the T. gondii B1 gene with the following primers described by Lin et al. (25) Toxo-F (5 µM; 5'-TCC CCT CTG CTG GCG AAA AGT-3') and Toxo-R (5 µM; 5'-AGC GTT, CGT GGT CAA CTA TCG ATT G-3). The target DNA for real-time PCR amplification was the published sequence of the 35-fold repetitive B1 gene of the RH strain (6). Template DNA (5 µl) was added to a reaction mixture (final volume, 25 µl) containing 0.75 U of Taq DNA polymerase (Platinum; Bio-Rad), 20 mM Tris-HCl, 50 mM KCl, 5 mM MgCl₂, 200 µM each dGTP, dATP, and dCTP, 400 µM dUTP, 0.5 U of UDG, 12.5 pmol of each primer, and 5 pmol of TaqMan fluorescent probe (2 µM; 5'FAM-TCT GTG CAA CTT TGG TGT ATT CGC AG-3'TAMRA). TaqMan PCR runs were performed in triplicate with an ICycler device (Bio-Rad). After initial activation of Taq polymerase at 95°C for 5 min, 45 PCR cycles were run at 95°C for 15 s and 60°C for 1 min. As the standard curve constructed with 10-fold serial-dilutions of purified T. gondii tachyzoites, this PCR was considered an end-point assay and so not appropriate for oocyst quantification. The PCR amplification was considered positive when DNA was detected in the three wells. To detect PCR inhibitors, DNA from a mimetic plasmid insert (corresponding to the target on the B1 gene deleted of nucleotides) was added in a second run in all DNA environmental samples, amplified with others primers, and revealed with SYBRgreen. When inhibitors were present (plasmid insert unamplified), 8 µg of bovine serum albumin (BSA; Boehringer, Mannheim, Germany) was added to a new reaction mixture before amplification (PCR/BSA).

(b) Bioassay.
We used a previously described procedure to induce the sporulation and infectivity of any T. gondii oocysts in the sediment (12). After addition of 5 ml of 2% H₂SO₄, the sediment was aerated at room temperature for 7 days. The suspension was neutralized by adding 3.3% sodium hydroxide and then centrifuged (10 min at 1,250 x g and 4°C). The supernatant was discarded, and the sediment was resuspended in 1.5 ml of normal saline containing antibiotics. Female Swiss-Webster mice (three mice per sample) were inoculated by gavage with well-mixed resuspended sample sediment. All mice were first confirmed to be seronegative for T. gondii. Blood was collected 6 weeks after infestation for serological analysis by high-sensitivity direct agglutination as previously described (31). Infection was demonstrated by seroconversion (specific immunoglobulin G antibody detection) and brain examination of sacrificed mice (2 months after inoculation).

Top Abstract Introduction Materials and Methods Results Discussion References

 
The results of PCR and bioassay detection of oocysts seeded in DW, PDW, and RSW are summarized in Table 1. PCR success rates in DW were 60% for the detection of 1 oocyst/liter and 100% for 10 oocysts/liter. The detection rate was 60% for 10 oocysts/liter in PDW and 50% for 1,000 oocysts/liter in RSW. The sensitivity of the PCR assay ranged from less than 10 to more than 1,000 oocysts/liter, depending on the source of the seeded sample. PCR was more sensitive than mouse inoculation. The detection rate at the bioassay detection limit in DW (1 oocyst/liter; Table 1) with the GES capsule was 30%. GES and GEHV capsules were evaluated for the recovery of T. gondii oocysts (Table 2). A 100-liter volume of DW seeded with 10³ oocysts was filtered at 1.5 liters/min using the two capsules. Samples were concentrated as described above and tested by PCR and bioassay. PCR success rates were 100% for the detection of 10 oocysts/liter in DW with the GES capsule, and 80% with the GEHV capsule. The positivity rate was 60% (three of five) with both capsules in the bioassay; two of five GES-filtered samples were totally negative in the bioassay, while only two of three mice were positive with the other three samples.

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TABLE 1. Water samplesa and results of PCR and bioassay

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TABLE 2. Comparison of the ability of GES and GEHV capsules to filter 100 liters of deionized water seeded with 103 T. gondii oocysts

A total of 139 water samples from 80 sites were tested by PCR and mouse inoculation. The turbidity of RSW samples ranged from 0.30 to 30.1 nephelometric turbidity units, while that of PDW samples ranged from 0.03 to 1.9 units. Among the 86 samples not containing PCR inhibitors, 9 were positive for Toxoplasma DNA and 77 were negative (Table 3). The other 53 samples contained PCR inhibitors. PCR-BSA overcame this inhibition in 39 cases (73.5%), leading to the detection of Toxoplasma DNA in one further positive sample. Inhibitors were more frequent in RSW (29 of 45; 64.4%) than in UW (18 of 50; 36%) or PDW (6 of 44; 13.6%). After PCR-BSA, only RSW (10 of 45; 22.2%) and UW (4 of 50; 8%) samples remained uninterpretable (principally samples with high turbidity).

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TABLE 3. DNA amplification by PCR or PCR-BSA in 139 samplesa

Finally, among the 125 interpretable samples, we detected Toxoplasma DNA in 10 cases (8%); 14 samples (10%; 10 RSW and 4 UW) were not amplified because of PCR inhibitors. None of the samples were positive by bioassay.

Top Abstract Introduction Materials and Methods Results Discussion References

 
T. gondii oocysts can persist for long periods in the environment. Experimental ingestion of a single oocyst can infect mice and pigs (12) while no data have been reported for human toxoplasmosis. T. gondii oocysts also exhibit remarkable resistance to various inactivation procedures based on chemical reagents (8, 9) and disinfection processes used by water utilities (42). The different methods for T. gondii oocyst recovery were recently reviewed (14). Standard methods currently available for detection of Cryptosporidium spp. and Giardia spp. in water include concentration-filtration of large volumes, elution and clarification on density gradients or by IMS, and immunofluorescence assay (IFA) using monoclonal antibodies (32). Here, we describe a rapid method for Toxoplasma detection in environmental water, including detection of Cryptosporidium spp. and Giardia spp. in the same sample.

The concentration-filtration step is critical and results in a marked loss of seeded oocysts (30). Recently, two chemical flocculation procedures and one centrifugation procedure were evaluated by Kourenti et al. for T. gondii oocyst concentration on DW, with recovery rates of more than 80% (23). While flocculation is simple and inexpensive, filtration is more robust for processing turbid water. Moreover, samples concentrated by filtration are less likely to contain PCR inhibitors, which appeared to be eliminated by using GES filters (28). For T. gondii, since oocyst numbers in random environmental samples are probably small, we used GES capsules to filter 7 to 45 liters of RSW and 100 liters of PDW. Since GEHV capsules permit the filtration of larger volumes (up to 1,000 liters), we also tested them with T. gondii-seeded samples. No major difference was found between the two capsules, and GEHV could thus be considered interesting for filtering larger volumes potentially containing T. gondii oocysts. The concentration-filtration process leads to the accumulation of debris in the filter, and oocyst detection requires clarification procedures to separate oocysts from debris (34). We used sucrose flotation which is commonly used for T. gondii oocyst purification (9, 12), since no monoclonal antibodies against the T. gondii oocyst outer wall are currently available (ruling out the use of IMS for concentration and IFA for quantitative detection).

Rapid and sensitive pathogen detection methods are essential for the public-water industry. PCR was described as more rapid, sensitive, and specific for Cryptosporidium species detection in environmental water samples (17, 19, 21); the sensitivity was found to be comparable for TaqMan PCR and conventional IFA (7). For DNA extraction, Sluter et al. (38) showed that three cycles of freezing-thawing were sufficient to expose Cryptosporidium oocyst DNA, resulting in higher sensitivity than proteinase K digestion or sonication. For T. gondii DNA extraction, we chose freezing-thawing for its speed, low cost, and simplicity. Nevertheless, PCR inhibitors may not be completely removed by flotation procedures and can compromise the sensitivity of molecular detection (5). Kreader (24) and Rochelle et al. (33) showed that BSA can be added to the PCR mix to avoid inhibition in samples containing humic acids (mixtures of complex polyphenolics produced during the decomposition of organic matter) (41). In our study, the use of PCR-BSA reduced the incidence of inhibitors from 38 to 10% of samples. The sensitivity of the PCR assay was reduced by up to 100-fold in oocyst-seeded RSW compared with DW and PDW. This is consistent with results from Johnson et al. (21) for PCR-based Cryptosporidium oocyst detection in water.

Finally, among the 125 interpretable samples, we detected Toxoplasma DNA in 10 cases (8%). Three cases involved RSW, whose environmental matrices may be contaminated by soil washing after peaks in rainfall (4). This could also be the case for the UW samples (six positive samples), which were chosen by local public health officials because of frequent pathogen recovery (including Giardia spp. and Cryptosporidium spp.). The detection of Toxoplasma DNA in PDW was more surprising, since none of the samples were positive by bioassay. In a previous study (20), T. gondii identification after filtration was based on mouse inoculation. Mouse bioassay is still the reference method to detect viable oocysts, but 7 days is required for sporulation, before mouse inoculation, and an additional 4 weeks is required to obtain the immunological results (20). As previously reported by Kourenti et al. (23), our seeding data suggest that Toxoplasma oocysts remain infective for mice. However, our bioassay results with environmental water samples were disappointing and showed that the efficiency of the bioassay for 10³ oocyst-seeded, & filtered, and eluted water samples was poor. Dubey et al. (12) and Isaac-Renton et al. (20), using the same method, failed to detect Toxoplasma oocysts in PDW. Previously, it was reported that the different isolation steps and vigorous shaking necessary for consistent oocyst elution may cause a loss of infectivity (35, 39). All these results show that while the mouse bioassay is still the reference test for viable oocysts, its efficiency is poor when it is applied to filtered environmental water samples. This could explain why none of our T. gondii PCR-positive samples were positive by bioassay. Another cause could be DNA contamination or detection of DNA from noninfective oocysts present in the environment. To avoid contamination, DNA extraction, PCR mix preparation, and PCR amplification were done in separated rooms. TaqMan PCR minimizes the possibility of cross-contamination because it involves a closed-vessel system and because of the presence of UDG in the mix (7). To distinguish between DNA from living and from dead oocysts, reverse transcription-PCR could be used as an important indirect technique for oocyst viability determination while it selectively detects viable organisms.

In conclusion, we describe here a strategy for the detection of multiple waterborne parasites, including Toxoplasma oocysts, in environmental water samples. PCR amplification was able to detect Toxoplasma DNA, even when the mouse bioassay was negative. These results suffer from some limitations, mainly owing to the flotation step. The development of monoclonal antibodies against the Toxoplasma oocyst wall would permit the use of IMS and also microscopic quantification by IFA. Moreover, efforts are under way in our laboratory to develop a quantitative reverse transcription-PCR method to differentiate between viable and nonviable oocysts detected in environmental samples since the mouse bioassay takes too long for public health sentinel purposes.

 
This work was supported by Ministère de l'Aménagement du Territoire et de l'Environnement (convention d'aide ENOOC12).

We thank the Communauté de Communes de l'Agglomération de Reims, the Conseil Regional and DRASS (Champagne-Ardenne), and the DDASS (Marne, Haute-Marne, Ardennes, Aube) for their cooperation in the collection of environmental water samples, and we thank Pall Life Science for providing GEHV capsules. We thank D. Young for editing the manuscript and M. L. Dardé for helpful discussions.

 
* Corresponding author. Mailing address: Laboratoire de Parasitologie-Mycologie, CHU Maison Blanche, 45 rue Cognacq-Jay, 51092 Reims, France. Phone: 00(0)3-26-78-42-20. Fax: 00(0)3-26-78-73-28. E-mail: ivillena{at}chu-reims.fr.

Top Abstract Introduction Materials and Methods Results Discussion References

 

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Applied and Environmental Microbiology, July 2004, p. 4035-4039, Vol. 70, No. 7
0099-2240/04/$08.00+0     DOI: 10.1128/AEM.70.7.4035-4039.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.

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