Open access

Molecular Detection and Genotyping of Toxoplasma gondii from Clinical Samples

Written By

Vladimir Ivovic, Marija Vujanic, Tijana Zivkovic, Ivana Klun and Olgica Djurkovic-Djakovic

Submitted: 05 June 2012 Published: 12 September 2012

DOI: 10.5772/50830

From the Edited Volume

Toxoplasmosis - Recent Advances

Edited by Olgica Djurković Djaković

Chapter metrics overview

4,785 Chapter Downloads

View Full Metrics

1. Introduction

Over the past two decades, molecular diagnosis of toxoplasmosis, which is based on the detection of T. gondii DNA in clinical samples, became an indispensable laboratory test. This method is independent of the immune response, and depending on methodological approach, may facilitate more accurate diagnosis, especially in cases in which inadequacy of conventional methods is faced with deteriorating and potentially severe clinical outcome (congenital, ocular toxoplasmosis and cases of immunosuppression).

Molecular methods based on polymerase chain reaction (PCR) are simple, sensitive, reproducible and can be applied to all clinical samples (Bell and Ranford-Cartwright, 2002; Contini et al., 2005; Calderaro et al., 2006; Bastien et al., 2007). These methods are divided into two groups. The first group consists of techniques focused on detection of T. gondii DNA in biological and clinical samples, including conventional PCR, nested PCR and real-time PCR. The second group consists of molecular methods including PCR-RFLP, microsatellite analysis and multilocus sequence typing of a single copy T. gondii DNA and those are predominantly used for strain typing (Su et al., 2010).

However, it is important to emphasize that molecular diagnostics, being a constantly improving modern methodology, is not standardized even among the world's leading laboratories. The differences are substantial and numerous, and they extend to all segments of the methodology such as target genes for parasite detection and markers for genotyping, equipment manufacturers and different protocols (various sets of primers and probes and their concentration, different internal controls, etc...).


2. Molecular diagnostics

2.1. Methodology

Conventional PCR was, in the beginning, the molecular detection method of choice for the majority of laboratories dealing with the diagnosis of toxoplasmosis and it was based on both in-house protocols and commercial kits (Lavrard et al., 1995). To increase the sensitivity of molecular diagnostics of toxoplasmosis nested PCR was introduced, although in recent years real-time PCR has shown a significantly higher sensitivity as well as specificity (Jauregui et al., 2001; Reischl et al., 2003; Contini et al., 2005; Calderaro et al., 2006; Edvinsson et al., 2006). Real-time PCR detection also has the capability of quantification of T. gondii in biological samples, which has found wide application in monitoring the kinetics and outcome of infection in patients undergoing therapy, as well as in experimental models (Lin et al., 2000; Jauregui et al., 2001; Contini et al., 2005; Djurković-Djaković et al., 2012).

Molecular diagnostics of toxoplasmosis is generally based on the detection of a specific DNA sequence, using different assays and protocols, mostly from highly conserved regions such as the B1 gene repeated 35 times in the genome, 529 bp repetitive element with about 200-300 copies in the genome, ITS-1 (internal transcribed spacer ) that exists in 110 copies and 18S rDNA gene sequences (Table 1). Qualitative PCR protocols for the detection of single copy genes such as the P30 gene appeared less sensitive and they are rarely used for diagnostic purposes (Jones et al., 2000).

MarkersNo. of copiesReferences
B1≈ 35Wahab et al., 2010
Correia et al., 2010
Okay et al., 2009
529 bp (AF146527)200-300da Silva RC et al., 2011
Yera et al., 2009
Vujanić et al., 2011
ITS-1 or 18S rDNA≈110Truppel et al., 2010
Miller et al., 2004
P30Single copy geneBuchbinder et al., 2003
Eida et al., 2009
Cardona et al., 2009

Table 1.

T. gondii DNA detection markers (latest and most significant data)

The first protocol for molecular detection of T. gondii, for conventional PCR targeting B1 gene, was developed in 1989 and has since been modified and optimized in many laboratories (Burg et al., 1989; Lopez et al., 1994; Liesenfeld et al., 1994; Reischl et al., 2003; Switaj et al., 2005). The B1 gene, although of unknown function, is widely exploited in a number of diagnostic and epidemiological studies because of its specificity and sensitivity. There are also some studies in which the detection of T. gondii parasites was based on amplification of ITS-1 and 18S rDNA fragments, whose sensitivity was similar to the B1 gene (Hurtado et al., 2001; Calderaro et al., 2006). However, the repetitive element of 529 bp in length, which was firstly identified by Homan, has showed a 10 to 100 times higher sensitivity compared to the B1 gene (Homan et al., 2000; Reischl et al., 2003). Nevertheless, there are several studies indicating that there are T. gondii strains in which either the whole or parts of the 529bp fragment have been deleted or mutated or in which the number of repeats vary. One report suggests that the 529bp repeat element, of unknown function as well, was not present in all isolates analyzed; 4.8% of the samples gave false-negative results compared to results from amplification of the B1 gene (Wahab et al. 2010.). Furthermore, some of the latest studies question its validity for quantification in clinical diagnostics since the number of copies of the 529 bp repetitive sequence in Toxoplasma genome appears to be 5 to 12 times lower than the previous estimations (Costa & Bretagne, 2012). Nevertheless, the detection of T. gondii DNA using the 529 bp repetitive element, and real-time PCR protocols that detect the presence of this element, is currently the most widely used molecular approach for the detection of T. gondii (Reischl et al., 2003; Kasper et al., 2009).

However, it can be of great methodological significance to further clarify the specificity of using a multicopy target of unknown function before the introduction of such protocol into the laboratory diagnostics (Edvinsson at al., 2006)

2.2. Clinical significance in various biological samples

Molecular detection of T. gondii in cases of suspected congenital toxoplasmosis may be performed in the amniotic fluid, and fetal and neonatal blood samples. Also, it is performed in the peripheral blood of immunosuppressed patients, and in samples of humor aqueous and cerebrospinal fluid of patients suspected of ocular and cerebral toxoplasmosis, as well as in bronchoalveolar lavage fluid (BAL). Furthermore, in our laboratory, peripheral blood of patients suspected of acute toxoplasmosis was also analyzed (Table 2).

Clinical sample Real-time PCR
No. testedNo. positive (%)
Blood9128 (30.8)
Amniotic fluid2810 (35.7)
Fetal blood93 (33.3)
BAL11 (100)
Aqueous humor106 (60)
Cerebrospinal fluid74 (57.1)
Total14652 (35.6)

Table 2.

Real-time PCR results on various clinical samples of patients suspected of active toxoplasmosis examined in the National Reference Laboratory for Toxoplasmosis, Belgrade, Serbia

2.2.1. Peripheral blood

In our laboratory, the presence of T. gondii DNA was shown in about one-third (31%) of all analysed cases. Similar research carried out on peripheral blood samples derived from patients with an acute T. gondii-related lymphadenopathy, resulted in the detection of parasite DNA in 35% of all samples (Guy & Joynson, 1995). In a study involving patients with acute toxoplasmosis in southeastern Brazil, the rate of parasite DNA-positive peripheral blood samples was 48.6% (17/35) (Kompalic-Cristo et al., 2007). Interestingly, both of these studies used B1 as the target gene, which is considered to be of lower sensitivity than the AF146527 marker that we used; however, the total number of analyzed samples was smaller and the patient selection criteria may have differed. In addition, in the Brazilian study DNA extraction was performed from the buffy coat instead of the whole blood, which may have contributed to the extraction of larger amounts of parasite DNA and higher success in its detection (Menotti et al., 2003; Jalal et al., 2004). Timely (early) sampling is also of particular importance, as detection of T. gondii DNA from the peripheral blood of patients with acute toxoplasmic lymphadenopathy has been shown to be very difficult 5.5 to 13 weeks after the onset of infection (Guy & Joynson, 1995). Successful PCR detection of T. gondii DNA should indicate recent infection. However, one must take into consideration that PCR detection of parasitic DNA alone does not necessarily mean that parasites are viable. The immune system rapidly kills circulating parasites but the T. gondii DNA could be retained for some period of time in the circulation. Also, it has been suggested that even in the chronic phase of infection it is possible, though very rarely, to detect in blood the DNA originating from cysts present in the muscles and nervous system (Guy & Joynson, 1995). On the other hand, negative PCR cannot exclude recent infection because of several reasons such as the small number of parasites circulating in the blood or short period of duration of parasitemia. Here it must be stressed that the exact kinetics of parasites in humans still remains unclear. Other reasons for negative PCR results include the small sample size from which DNA is extracted compared to the total volume of blood in the human body, as well as the fact that the blood contains components that may inhibit the PCR reaction, primarily heme, hemoglobin, lactoferrin and immunoglobulin G.

We have analyzed real-time PCR results from peripheral blood samples originating from patients suspected of acute toxoplasmosis according to the serological criteria for acute infection, i.e. avidity of specific IgG antibodies and the finding of specific IgM antibodies. The results showed that positive real-time PCR correlates better with the finding of specific IgM antibodies, than with low avidity of specific IgG antibodies (Vujanić, 2012).

Comparison of molecular detection and bioassay findings on peripheral blood samples of the patients with specific IgM antibodies and specific IgG antibodies of low avidity, suggesting acute toxoplasmosis, has been done as well. It was shown that in nearly one-third (29%) of the analyzed cases T. gondii DNA was detected in comparison to approximately 20% positive bioassays. This result undoubtedly indicates a higher sensitivity of the real-time PCR method in relation to the bioassay. However, molecular detection of parasite DNA in peripheral blood is of the greatest significance in immunosuppressed patients, where it may be the only method for both the diagnosis and monitoring of the therapeutic effect of the administered antiparasitic drugs. The significance of real-time PCR for monitoring the kinetics of the infection has been shown in immunosuppressed patients after bone marrow and liver transplantation (Costa et al., 2000; Botterel et al., 2002 ; Edvinsson et al., 2008; Daval et al., 2010). Using real-time PCR, we too have observed a decline in parasitemia in a patient with reactivated toxoplasmosis during specific treatment (Vujanić 2012).

Although the detection of parasite DNA in peripheral blood of adults may not always be direct evidence of active parasitemia, T. gondii DNA detected in fetal and neonatal blood samples is of the utmost clinical importance because there is no possibility of detection of DNA from earlier infections. Therefore, the most important application of molecular methods is in the diagnosis of congenital toxoplasmosis, as the isolation of the parasite in cell culture is insufficiently sensitive (Thulliez et al., 1992; Foulon et al., 1999) and the isolation by bioassay takes approximately 6 weeks.

2.2.2. Amniotic fluid

In the last two decades, the detection of T. gondii DNA in the amniotic fluid has become particularly important, as it allows for timely diagnosis of fetal infection, and subsequent implementation of appropriate therapy and infection control (Menotti et al., 2010; Wallon et al., 2010). We have so far studied a total of 28 amniotic fluid samples obtained from women suspected of infection in pregnancy. Real-time PCR revealed parasite DNA in 36% of the amniotic fluid samples whereas mouse bioassay was positive in 25%. A similar difference in the positivity rate between PCR (17/85, 20%) and bioassay (14/85, 16.5%) results was obtained in a study in Egypt (Eida et al., 2009).

Given that in many published studies real-time PCR and bioassay results from the amniotic fluid did not match, which is the case in our research as well, and as congenital infection cannot be excluded by negative PCR (Romand et al., 2001; Golab et al., 2002), for prediction of congenital toxoplasmosis it is optimal to combine both molecular detection and bioassay. In one study of prenatal diagnosis of congenital toxoplasmosis in patients from 6 European centers of reference it was shown that PCR from amniotic fluid has a higher sensitivity (81%) in regard to both bioassay (58%) and cell culture (15%) (Foulon et al., 1999). The combination of PCR and bioassay increases the sensitivity to 91%, and represents the best diagnostic approach (Foulon et al., 1999).

In European countries such as France and Austria regular serological monitoring of pregnant women for T. gondii is regulated by law, which allows for precise timing of seroconversion and timely prenatal diagnosis of fetal infection. This has also allowed for a vast experience with the diagnosis of congenital toxoplasmosis, and provided data on the superior sensitivity of molecular methods compared to conventional parasitological tests. Thus, one long-term study conducted in France showed that out of 2632 women in whom the infection occurred during pregnancy, congenital toxoplasmosis was confirmed by positive PCR in the amniotic fluid and/or fetal blood in 34 cases in which congenital infection was diagnosed by conventional methods, as well as in three fetuses in whom the infection was not diagnosed by other methods (Hohlfeld et al., 1994). Also, in a similar study in Austria, outcome of prenatally diagnosed children was followed-up during the first year of life to assess the validity of PCR results from the amniotic fluid. Of the 49 amniotic fluid samples analyzed, congenital infection was confirmed postnatally by serological monitoring in all 11 (22.4%) PCR-positive ones, whereas none of the 38 children in whom PCR of the amniotic fluid was negative was shown to be infected (Gratzl et al., 1998).

2.2.3. Cord blood

Cord blood is not considered the ideal sample for prenatal diagnosis of congenital toxoplasmosis. For example, the results of a survey carried out in France did not show any positive PCR result among 19 tested cord blood samples from children with proven congenital toxoplasmosis (Filisetti et al., 2003). Nevertheless, cord blood samples that are occasionally provided to our laboratory, have shown a rate of positivity in real-time PCR of 33%. All cord blood samples in our study were inoculated into mice and the rate of positivity of bioassay was 55.5%. A higher rate of isolation of viable parasites by bioassay compared to the detection of parasitic DNA by real-time PCR may be explained by a larger sample volume used for mouse inoculation in comparison to the amount used for DNA extraction, as well as by probable presence of PCR inhibitors. In one study performed on a representative sample of pregnant women in China a similar rate of real-time PCR positive results was obtained from the amniotic fluid and fetal blood samples (Ma et al., 2003).

It can be concluded that the diagnosis of congenital toxoplasmosis from fetal blood samples should be based on the results of both bioassay and molecular detection.

2.2.4. Aqueous humor

Prior to the introduction of molecular methods, the laboratory diagnosis of ocular toxoplasmosis has been based primarily on a comparison of the level of antibodies detected in the humor aqueous and serum in order to detect intraocular synthesis of specific antibodies (Witmer-Goldman's coefficient). Lately, molecular methods are becoming a standard diagnostic approach in the diagnosis of ocular toxoplasmosis as well. A number of studies has already shown that a positive PCR result is not always accompanied by positive serology indicating local synthesis of IgG antibodies (Villard et al., 2003; Talabani et al., 2009) and thus can be the only confirmation of the diagnosis (Okhravi et al., 2005).

We have so far studied 10 humor aqueous samples from patients clinically suspected of ocular toxoplasmosis of which 60% (6/10) were real-Time PCR positive. A similar result was obtained in a French study when 55% (22/40) of humor aqueous samples were positive by real-Time PCR using AF146527 as a marker (Talabani et al., 2009). Also, the detection of the same AF146527 marker by real-Time PCR in another French study, revealed somewhat lower rate of positive samples, 38.2% (13/34) (Fekkar et al., 2008). It is interesting that in the latter study the sample volume of 10 μL used for DNA extraction was unusually small, which certainly could affect the success of PCR reactions. However, in another study performed in Strasbourg, the amplification of 18S rRNA and B1 gene by conventional PCR resulted in the 28% (5/18) of the humor aqueous samples positive for the presence of T. gondii DNA (Villard et al., 2003).

2.2.5. Cerebrospinal fluid

Cerebral toxoplasmosis usually affects immunosuppressed patients and is mostly the result of reactivation of chronic infection which may be fatal if left untreated. Definitive diagnosis of toxoplasmosis can be made by the detection of tachyzoites in brain tissue samples obtained by biopsy, but this method, because of its invasiveness, is seldom applied, and certainly not since the PCR, giving consistent and quick result, has been introduced in the diagnostics (Vidal et al., 2004). A study of cerebral toxoplasmosis in HIV-infected patients infected in Brazil, showed that 27.4% (14/51) of cerebrospinal fluid samples were positive for T. gondii DNA (Mesquita et al., 2010). Noteworthy, DNA extraction was performed using phenol-chloroform method, in which the phenolic residues can often inhibit the PCR reaction. In our limited experience, of the 7 cerebrospinal fluid samples obtained from patients with different neurological conditions (including one case of congenital hydrocephalus) examined by real-time PCR, 4 (57%) were positive.

2.3. Comment

In summary, all above-mentioned results confirm the value of the use of molecular methods, due to their high sensitivity and specificity, in the diagnosis of toxoplasmosis. Coupled with conventional parasitological diagnostic methods, PCR-based methods allow for the timely diagnosis especially of congenital toxoplasmosis and of reactivated toxoplasmosis in immunosuppressed patients. Further advances of the technology itself along with its wide, (universal) use may be expected to markedly improve diagnostics and monitoring of the course of infection as well as of the therapeutic effect.


3. Genotyping

In the early days of strain designation, isolates of T. gondii have been grouped according to virulence in outbred mice. First phylogenetic studies of T. gondii strains indicated that their genetic complexity was much smaller than expected (Darde et al., 1992; Sibley & Boothroyd, 1992). Howe and Sibley’s T. gondii population structure study (1995) performed on 106 isolates collected from both humans and animals from North America and Europe, showed the presence of three clonal types (type I, II and III) and very small differences between clonal lineages which is why it was concluded that T. gondii has a clonal population structure. Comparative sequence analysis of individual genes indicated extremely low allelic diversity within the clonal lines, and only 1% divergence at the DNA level. In addition, limited genetic diversity between and within clonal lines indicated that they have quite recently evolved from a common ancestor, 10,000 years ago at the most (Su et al., 2003).

Nevertheless, most recent phylogenetic studies indicate that the population structure of T. gondii is much more complex than initially considered. While it has been undeniably established that type II is predominant in Europe and North America (Darde et al., 1992; Howe & Sibley, 1995; Howe et al., 1997), there are significant regional differences. Thus, research in Portugal and Spain showed the presence of types I and III in this area (Fuentes et al., 2001; de Sousa et al., 2006), while genotyping of isolates from Crete and Cyprus showed the predominance of type III (Messaritakis et al., 2008); however it must be noted that these studies have been conducted using only one marker (SAG2 or GRA6). Also, phylogenetic analyses of T. gondii isolates, which have only recently begun in South America, Asia and Africa, have shown considerable genetic diversity of this parasite strains.

A realistic picture of the distribution of genotypes in Europe is also difficult to obtain because research on T. gondii is not performed to the same extent and using the same methods in all geographical areas. So far, the largest number of isolates has been genotyped in France, mainly thanks to the mandatory program of testing of pregnant women for toxoplasmosis in this country, which allows for the availability of research material. One French study has shown that of the 86 isolates from cases of suspected and confirmed congenital toxoplasmosis 85% were of type II (Ajzenberg et al., 2002). A predominance of the same type was indicated in Poland, where genotyping was also performed in samples originating from clinical cases of congenital toxoplasmosis (Nowakowska et al., 2006). In South-East Europe the first strain genotyped was isolated from a case of congenital toxoplasmosis in Serbia, and was also designated as type II (Djurković-Djaković et al., 2006).

Further work on the genotyping of T. gondii strains in Serbia showed another two type II isolates, originating from a case of congenital toxoplasmosis and a case of toxoplasmosis in pregnancy, respectively. However, another isolate from a peripheral blood sample of a neonate with suspected congenital toxoplasmosis had been typed to the clonal type I. Isolation of this genotype from cases of congenital toxoplasmosis has been described, but at a significantly lower rate than type II (Howe & Sibley, 1995), as results of research conducted in France have shown, where out of 86 genotyped isolates only 4 belonged to type I (Ajzenberg et al., 2002).

Sample numberSample typeClinical entityGenotype
1bloodtoxoplasmosis in pregnancyII
2amniotic fluidcongenital toxoplasmosisII
3bloodcongenital toxoplasmosisI
4*bloodbone marrow transplantationII
5*bronchoalveolar lavage fluidbone marrow transplantationII

Table 3.

Genotypes of human T. gondii isolates from clinical samples in Serbia

We have also genotyped isolates from both a blood and BAL sample from an immunosuppressed patient after bone marrow transplantation, which were found to belong to type II. In another study, genotyping of strains isolated from immunosuppressed patients, HIV infected or patients who had undergone organ transplantation, has shown predominance of type II in patients who were infected in Europe (Ajzenberg et al., 2009). On the other hand, isolates that do not belong to this type usually come from people who are infected with T. gondii out of Europe. In this group of patients type III was the second in abundance whereas type I was rare (Ajzenberg et al., 2009). In other studies carried out in immunosuppressed patients (patients with AIDS, lymphoma or patients with transplants), which mainly came from France, it was shown that type II isolates were also predominant, while types I and III were isolated rarely (Howe et al., 1997; Honore et al., 2000).

Furthermore, results of a study performed in the USA, based on genotyping of strains isolated from cerebrospinal fluid originating from eight HIV-positive patients showed that most of them were infected with type I strain or strains that have type I alleles (Khan et al., 2005). Although the possible association between clinical entities induced by T. gondii with specific T. gondii genotypes is yet unclear, it is likely that the resistance or susceptibility to a particular type, especially in immunosuppressed patients, is primarily dependent on individual factors (Ajzenberg et al., 2009). The greatest limitation in genotyping of isolates from clinical samples is the small number of parasites in original material; hence the amount of extracted T. gondii DNA is often also small. This problem can be partially eliminated by enriching the sample by bioassay or cell culture, but even the most sensitive molecular methods, such as a multiplex nested PCR, have a threshold of 50 and 25 parasites/mL, respectively (Khan et al., 2005; Nowakowska et al., 2006). The PCR-RFLP protocol by which genotyping was performed in our study has a sensitivity of approximately 170 parasites/mL, which is probably the major reason for the small number of successful genotypizations.

Numerous studies of the T. gondii population structure were based on genotyping using a single marker, mostly SAG2 (Howe et al., 1997; Fuentes et al., 2001; Sabaj et al., 2010) and particularly, due to its polymorphisms and sensitivity, GRA6 (Fazaeli et al., 2000; Messaritakis et al., 2008). However, genotyping with a single marker does not allow identification of nonclonal strains, and to determine more precisely the presence of polymorphisms in the population, application of multilocus PCR-RFLP and microsatellite analysis of multiple markers is necessary (Ajzenberg et al., 2005; Su et al., 2006). Although in our experience the GRA6 gene was, due to a small amount of T. gondii DNA, the only amplified marker in a blood sample of a neonate suspected of congenital toxoplasmosis (Table 3), that clearly indicated the presence of type I, in our laboratory genotyping is regularly performed using SAG1, SAG2, GRA6 and GRA7 as markers (Miller et al., 2004; Dubey et al., 2007; Prestrud et al., 2008; Richomme et al., 2009; Aubert et al., 2010).

But even the use of multiple markers does not always provide satisfactory results, mainly due to insufficient amounts of extracted parasite DNA. Therefore, there are cases when amplification of all markers in each sample is not successful, as it can be observed in studies performed in the United States and Poland, where PCR-RFLP analysis was carried out also using four genetic markers SAG2, SAG3, BTUB and GRA6 (Khan et al., 2005; Nowakowska et al., 2006). Using these genetic markers, it was possible to discriminate types I, II and III, but also strains that have a genotype with two allele types at the same locus. Such was the case with one sample in our study which, after the digestion of the product of the amplified GRA7 gene, turned out to possess alleles of both types I and II (Fig. 1, Mbo II and Eco RI).

Although PCR-RFLP has a limited ability to distinguish between closely related isolates within a clonal line as compared to microsatellite analysis, analysis of up to 9 or 10 genetic markers by this method has been successfully performed in world-class laboratories (Su et al., 2006; Dubey & Su, 2009). On the other hand, the microsatellite analysis is presumed to be more informative to distinguish recent mutations in closely related isolates of the same line, while the RFLP markers are better for detection of time period when the separation of distinct strains in different clonal group has occurred (Su et al., 2006). Multilocus PCR-RFLP genotyping is still the first method of choice in clinical research, mainly for its simplicity and favorable reagent prices, but the best approach for successful genotyping is the use of both methods.

Figure 1.

Genotyping pattern summary (markers and restriction enzymes used in genotyping protocol) – illustrative example

Along with the phylogenetic study of T. gondii, there is ongoing research aimed at explaining the possible link between the different genotypes and clinical forms of the disease. In spite of the results indicating lack of connection, or a much more complex one than some studies show, there are reported findings on population structure of T. gondii that are likely to have important clinical implications. Although it is generally accepted that type II is predominant in cases of congenital toxoplasmosis, at least in Europe and North America (Howe & Sibley, 1995; Howe et al., 1997; Ajzenberg et al., 2002; Darde et al., 2007), type I strains may also be associated with some severe forms of the disease (Howe et al., 1997; Fuentes et al., 2001). Furthermore, strains of atypical genotypes were isolated from immunocompetent patients with severe acquired toxoplasmosis in French Guiana (Carme et al., 2002; Demar et al., 2011), whereas type I and some recombinant strains were isolated from immunocompetent individuals suffering from severe or atypical ocular toxoplasmosis in United States (Grigg et al., 2001).

Even the generally accepted concept of major clinical importance that immunized mothers are resistant to reinfection thereby preventing infection of the offspring, have been recently challenged by insight into the strain variation at the genotype level. Six cases of reinfection among chronically infected pregnant women resulting in a vertical transmission and congenital infection either with a distinct typical or atypical strain have already been reported (Lindsay & Dubey, 2011).

Despite this significant new knowledge, the clinical relevance of the infecting genotypes is an issue that will continue to intrigue researchers in the coming years. Insight into the global population structure of T. gondii and its clinical implications, complicated by the growing rate of human migrations among continents, will require wide research efforts based on more standardized protocols, and should include not only clinically manifest cases, but also individuals with asymptomatic infection.


4. Conclusion

The introduction of highly sensitive molecular methods into the diagnosis of toxoplasmosis is of great importance and this paper emphasizes its practical importance and potential as a part of the standard laboratory protocols. Nevertheless, it can be concluded that, at the moment, the best diagnostic approach is a combination of both conventional and molecular methods.

We also present the very first and original phylogenetic data on the T. gondii population structure in Serbia. It is shown that in this area, as much as in the rest of the Europe, a clonal population structure is characterized by the predominance of genotype II and much less of genotype I. However, given the fact that the whole region of the Balkan Peninsula is an area of contact with Asia and Africa, where the T. gondii population structure is rather different, one may expect a larger diversity, including the presence of clonal type III or even atypical strains, particularly in wild animals.


The work was supported by a grant (project No. III41019) from the Ministry of Education and Science of Serbia.


  1. 1. AjzenbergD.CogneN.ParisL.BessieresM. H.ThulliezP.FilisettiD.PellouxH.MartyP.DardeM. L.2002Genotype of 86 Toxoplasma gondii isolates associated with human congenital toxoplasmosis, and correlation with clinical findings. J Infect Dis 186, 5: 684 EOF9 EOF
  2. 2. AjzenbergD.DumetreA.DardeM. L.2005Multiplex PCR for typing strains of Toxoplasma gondii. J Clin Microbiol 43, 4: 1940 EOF3 EOF
  3. 3. AjzenbergD.YeraH.MartyP.ParisL.DalleF.MenottiJ.AubertD.FranckJ.BessieresM. H.QuinioD.PellouxH.DelhaesL.DesboisN.ThulliezP.Robert-GangneuxF.Kauffmann-LacroixC.PujolS.RabodonirinaM.MEBougnouxCuisenier. B.DuhamelC.DuongT. H.FilisettiD.FloriP.Gay-AndrieuF.PratlongF.NevezG.TotetA.CarmeB.BonnabauH.DardeM. L.VillenaI.2009Genotype of 88 Toxoplasma gondii isolates associated with toxoplasmosis in immunocompromised patients and correlation with clinical findings. J Infect Dis 199, 8: 1155 EOF67 EOF
  4. 4. AubertD.AjzenbergD.RichommeC.Gilot-FromontE.METerrier deGevigney. C.GameY.MaillardD.GibertP.DardeM. L.VillenaI.2010Molecular and biological characteristics of Toxoplasma gondii isolates from wildlife in France. Vet Parasitol 171, 3-4: 346 EOF349 EOF
  5. 5. BastienP.Jumas-BilakE.Varlet-MarieE.MartyP.2007Three years of multi-laboratory external quality control for the molecular detection of Toxoplasma gondii in amniotic fluid in France. Clin Microbiol Infect 13, 4: 430 EOF433 EOF
  6. 6. BellA.Ranford-CartwrightL.2002Real-time quantitative PCR in parasitology. Trends Parasitol 18, 8: 338.
  7. 7. BotterelF.IchaiP.FerayC.BoureeP.SalibaF.TurRaspa. R.SamuelD.RomandS.2002Disseminated toxoplasmosis, resulting from infection of allograft, after orthotopic liver transplantation: usefulness of quantitative PCR. J Clin Microbiol 40, 5:1648 EOF50 EOF
  8. 8. BuchbinderS.BlatzR.RodloffA. C.2003Comparison of real-time PCR detection methods for B1 and 30genes of Toxoplasma gondii. Diagn Microbiol Infect Dis 45, 4: 269-271.
  9. 9. BurgJ. L.GroverC. M.PoulettyP.BoothroydJ. C.1989Direct and sensitive detection of a pathogenic protozoan, Toxoplasma gondii, by polymerase chain reaction. J Clin Microbiol 27, 8: 1787 EOF92 EOF
  10. 10. CaldearoA.PiccoloG.GorriniC.PeruzziS.ZerbiniL.BommezzadriS.DettoriG.ChezziC.2006Comparison between two real-time PCR assays and a nested-PCR for the detection of Toxoplasma gondii. Acta Biomed 77, 2: 75-80.
  11. 11. E.2009Toxoplasma gondii: 30peptides recognition pattern in human toxoplasmosis. Exp Parasitol 123, 2: 199-202.
  12. 12. CarmeB.BissuelF.AjzenbergD.BouyneR.AznarC.DemarM.BichatS.LouvelD.BourbigotA. M.PeneauC.NeronP.DardeM. L.2002Severe acquired toxoplasmosis in immunocompetent adult patients in French Guiana. J Clin Microbiol 40, 11: 4037 EOF44 EOF
  13. 13. ContiniC.SeraceniS.CultreraR.IncorvaiaC.SebastianiA.PicotS.2005Evaluation of a Real-time PCR-based assay using the lightcycler system for detection of Toxoplasma gondii bradyzoite genes in blood specimens from patients with toxoplasmic retinochoroiditis. Int J Parasitol 35, 3: 275 EOF83 EOF
  14. 14. Correia CC, Melo HR, Costa VM2010Influence of neurotoxoplasmosis characteristics on real-time PCR sensitivity among AIDS patients in Brazil. Trans R Soc Trop Med Hyg 104, 1: 24 EOF28 EOF
  15. 15. CostaJ. M.BretagneS.2012Variation of B1 gene and AF146527 repeat element copy numbers according to Toxoplasma gondii strains assessed using real-time quantitative PCR. J Clin Microbiol 50, 4: 1452 EOF1454 EOF
  16. 16. CostaJ. M.PautasC.ErnaultP.FouletF.CordonnierC.BretagneS.2000Real-time PCR for diagnosis and follow-up of Toxoplasma reactivation after allogeneic stem cell transplantation using fluorescence resonance energy transfer hybridization probes. J Clin Microbiol 38, 8: 2929 EOF32 EOF
  17. 17. DardeM. L.BouteilleB.Pestre-AlexandreM.1992Isoenzyme analysis of 35 Toxoplasma gondii isolates and the biological and epidemiological implications. J Parasitol 78, 5: 786 EOF
  18. 18. DardeM.AjzenbergD.SmithJ.2007Population Structure and Epidemiology of Toxoplasma gondii. In: Weiss, L.M., Kim, K. (Eds.) Toxoplasma gondii The Model Apicomplexan: Perspectives and Methods. Elsevier, 4976
  19. 19. DavalS.PoirierP.ArmenaudJ.CambonM.LivrelliV.2010Development of a real-time PCR assay for quantitative diagnosis of Toxoplasma gondii after allogeneic bone marrow transplantation]. Pathol Biol (Paris) 58, 1: 104 EOF9 EOF
  20. 20. DemarM.HommelD.DjossouF.PeneauC.BoukhariR.LouvelD.BourbigotA. M.NasserV.AjzenbergD.DardeM. L.CarmeB.2011Acute toxoplasmoses in immunocompetent patients hospitalized in an intensive care unit in French Guiana. Clin Microbiol Infect doi:j.14690691x.
  21. 21. Djurković-DjakovićO.DjokićV.VujanićM.ZivkovićT.BobićB.NikolićA.SlavićK.KlunI.IvovićV.2012Kinetics of parasite burdens in blood and tissues during murine toxoplasmosis. Exp Parasitol 131, 3: 372 EOF376 EOF
  22. 22. Djurkovic-DjakovicO.KlunI.KhanA.NikolicA.Knezevic-UsajS.BobicB.SibleyL. D.2006A human origin type II strain of Toxoplasma gondii causing severe encephalitis in mice. Microbes Infect 8, 8: 2206 EOF2212 EOF
  23. 23. DubeyJ. P.SuC.2009Population biology of Toxoplasma gondii: what’s out and where did they come from. Mem Inst Oswaldo Cruz 104, 2: 190 EOF195 EOF
  24. 24. DubeyJ. P.SundarN.GennariS. M.MinervinoA. H.FariasN. A.RuasJ. L.dosSantos. T. R.CavalcanteG. T.KwokO. C.SuC.2007Biologic and genetic comparison of Toxoplasma gondii isolates in free-range chickens from the northern Para state and the southern state Rio Grande do Sul, Brazil revealed highly diverse and distinct parasite populations. Vet Parasitol 143, 2: 182 EOF188 EOF
  25. 25. EdvinssonB.LappalainenM.EvengardB.2006Real-time PCR targeting a 529bp repeat element for diagnosis of toxoplasmosis. Clin Microbiol Infect 12, 2: 131-136.
  26. 26. EdvinssonB.LundquistJ.LjungmanP.RingdenO.EvengardB.2008A prospective study of diagnosis of Toxoplasma gondii infection after bone marrow transplantation. APMIS 116, 5: 345 EOF351 EOF
  27. 27. Eida OM, Eida MM, Ahmed AB2009Evaluation of polymerase chain reaction on amniotic fluid for diagnosis of congenital toxoplasmosis. J Egypt Soc Parasitol 39, 2: 541 EOF50 EOF
  28. 28. FazaeliA.CarterP. E.DardeM. L.PenningtonT. H.2000Molecular typing of Toxoplasma gondii strains by GRA6 gene sequence analysis. Int J Parasitol 30, 5: 637 EOF42 EOF
  29. 29. FekkarA.BodaghiB.TouafekF.Le HoangP.MazierD.ParisL.2008Comparison of immunoblotting, calculation of the Goldmann-Witmer coefficient, and real-time PCR using aqueous humor samples for diagnosis of ocular toxoplasmosis. J Clin Microbiol 46, 6: 1965 EOF1967 EOF
  30. 30. FilisettiD.GorciiM.Pernot-MarinoE.VillardO.CandolfiE.2003Diagnosis of congenital toxoplasmosis: comparison of targets for detection of Toxoplasma gondii by PCR. J Clin Microbiol 41, 10: 4826 EOF8 EOF
  31. 31. FoulonW.PinonJ. M.Stray-PedersenB.PollakA.LappalainenM.DecosterA.VillenaI.JenumP. A.HaydeM.NaessensA.1999Prenatal diagnosis of congenital toxoplasmosis: a multicenter evaluation of different diagnostic parameters. Am J Obstet Gynecol 181, 4: 843-847.
  32. 32. FuentesI.RubioJ. M.RamirezC.AlvarJ.2001Genotypic characterization of Toxoplasma gondii strains associated with human toxoplasmosis in Spain: direct analysis from clinical samples. J Clin Microbiol 39, 4: 1566 EOF70 EOF
  33. 33. GuyE.JoysonD.1995Potential of the Polymerase Chain Reaction in the Diagnosis of Active Toxoplasma Infection by Detection of Parasite in Blood. J Infect Dis 172, 1: 319 EOF22 EOF
  34. 34. GolabE.NowakowskaD.WalochM.DzbenskiT. H.SzaflikK.WilczynskiJ.2002Detection of congenital toxoplasmosis in utero with a polymerase chain reaction on amniotic fluid]. Wiad Parazytol 48, 3: 311 EOF5 EOF
  35. 35. GratzlR.HaydeM.KohlhauserC.HermonM.BurdaG.StroblW.PollakA.1998Follow-up of infants with congenital toxoplasmosis detected by polymerase chain reaction analysis of amniotic fluid. Eur J Clin Microbiol Infect Dis 17, 12: 853 EOF8 EOF
  36. 36. MEGriggGanatra. J.BoothroydJ. C.MargolisT. P.2001Unusual abundance of atypical strains associated with human ocular toxoplasmosis. J Infect Dis 184, 5: 633 EOF9 EOF
  37. 37. HohlfeldP.DaffosF.CostaJ. M.ThulliezP.ForestierF.VidaudM.1994Prenatal diagnosis of congenital toxoplasmosis with a polymerase-chain-reaction test on amniotic fluid. N Engl J Med 331, 11: 695 EOF9 EOF
  38. 38. HomanW. L.VercammenM.De BraekeleerJ.VerschuerenH.2000Identification of a 200to 300-fold repetitive 529 bp DNA fragment in Toxoplasma gondii, and its use for diagnostic and quantitative PCR. Int J Parasitol 30, 1: 69-75.
  39. 39. HonoreS.CouvelardA.GarinY. J.BedelC.HeninD.DardeM. L.DerouinF.2000Genotyping of Toxoplasma gondii strains from immunocompromised patients]. Pathol Biol (Paris) 48, 6: 541 EOF7 EOF
  40. 40. Howe DK, Sibley LD1995Toxoplasma gondii comprises three clonal lineages: correlation of parasite genotype with human disease. J Infect Dis 172, 6: 1561 EOF6 EOF
  41. 41. HoweD. K.HonoreS.DerouinF.SibleyL. D.1997Determination of genotypes of Toxoplasma gondii strains isolated from patients with toxoplasmosis. J Clin Microbiol 35, 6: 1411 EOF4 EOF
  42. 42. HurtadoA.AdurizG.MorenoB.BarandikaJ.Garcia-PerezA. L.2001Single tube nested PCR for the detection of Toxoplasma gondii in fetal tissues from naturally aborted ewes. Vet Parasitol 102, 1-2: 17 EOF27 EOF
  43. 43. JalalS.CENordLappalainen. M.EvengardB.2004Rapid and sensitive diagnosis of Toxoplasma gondii infections by PCR. Clin Microbiol Infect 10, 10: 937 EOF939 EOF
  44. 44. JaureguiL. H.HigginsJ.ZarlengaD.DubeyJ. P.LunneyJ. K.2001Development of a real-time PCR assay for detection of Toxoplasma gondii in pig and mouse tissues. J Clin Microbiol 39, 6: 2065 EOF71 EOF
  45. 45. JonesC. D.OkhraviN.AdamsonP.TaskerS.LightmanS.2000Comparison of PCR detection methods for B1, 30and 18S rDNA genes of T. gondii in aqueous humor. Invest Ophthalmol Vis Sci 41, 3: 634-644.
  46. 46. KasperD. C.SadeghiK.PrusaA. R.ReischerG. H.KratochwillK.Forster-WaldlE.GerstlN.HaydeM.PollakA.HerknerK. R.2009Quantitative real-time polymerase chain reaction for the accurate detection of Toxoplasma gondii in amniotic fluid. Diagn Microbiol Infect Dis 63, 1: 10 EOF15 EOF
  47. 47. KhanA.SuC.GermanM.StorchG. A.CliffordD. B.SibleyL. D.2005Genotyping of Toxoplasma gondii strains from immunocompromised patients reveals high prevalence of type I strains. J Clin Microbiol 43, 12: 5881 EOF7 EOF
  48. 48. Kompalic-CristoA.FrottaC.Suarez-MutisM.FernandesO.BrittoC.2007Evaluation of a real-time PCR assay based on the repetitive B1 gene for the detection of Toxoplasma gondii in human peripheral blood. Parasitol Res 101, 3: 619 EOF625 EOF
  49. 49. LavrardI.ChouaidC.RouxP.PoirotJ. L.MarteauM.LemarchandB.MeyohasM. C.OlivierJ. L.1995Pulmonary toxoplasmosis in HIV-infected patients: usefulness of polymerase chain reaction and cell culture. Eur Respir J 8, 5: 697 EOF700 EOF
  50. 50. LiesenfeldO.RothA.WeinkeT.FossH. D.HahnH.1994A case of disseminated toxoplasmosis-value of PCR for the diagnosis. J Infect 29, 2: 133 EOF8 EOF
  51. 51. Lin MH, Chen TC, Kuo TT, Tseng CC, Tseng CP2000Real-time PCR for quantitative detection of Toxoplasma gondii. J Clin Microbiol 38, 11: 4121 EOF5 EOF
  52. 52. Lindsay DS, Dubey JP2011Toxoplasma gondii: the changing paradigm of congenital toxoplasmosis. Parasitology 138, 14: 1829 EOF1831 EOF
  53. 53. MaMuY. Y.WangR. L.JiangL. Y.S.2003Study on prenatal diagnosis using fluorescence quantitative polymerase chain reaction for congenital toxoplasmosis]. Zhonghua Fu Chan Ke Za Zhi 38 EOF10 EOF
  54. 54. MenottiJ.GarinY. J.ThulliezP.SerugueM. CastroN.HouzeS.DerouinF.2010Evaluation of a new 5’-nuclease real-time PCR assay targeting the Toxoplasma gondii AF146527 genomic repeat. Clin Microbiol Infect 16, 4: 363 EOF8 EOF
  55. 55. MenottiJ.VilelaG.RomandS.GarinY. J.AdesL.GluckmanE.DerouinF.RibaudP.2003Comparison of PCR-enzyme-linked immunosorbent assay and real-time PCR assay for diagnosis of an unusual case of cerebral toxoplasmosis in a stem cell transplant recipient. J Clin Microbiol 41, 11: 5313 EOF6 EOF
  56. 56. Mesquita RT, Ziegler AP, Hiramoto RM, Vidal JE, Pereira-Chioccola VL2010Real-time quantitative PCR in cerebral toxoplasmosis diagnosis of Brazilian human immunodeficiency virus-infected patients. J Med Microbiol 59, 6: 641 EOF647 EOF
  57. 57. MessaritakisI.DetsikaM.KoliouM.SifakisS.AntoniouM.2008Prevalent genotypes of Toxoplasma gondii in pregnant women and patients from Crete and Cyprus. Am J Trop Med Hyg 79, 2: 205 EOF9 EOF
  58. 58. MAMillerGrigg.MEKreuderC.JamesE. R.MelliA. C.CrosbieP. R.JessupD. A.BoothroydJ. C.BrownsteinD.ConradP. A.2004An unusual genotype of Toxoplasma gondii is common in California sea otters (Enhydra lutris nereis) and is a cause of mortality. Int J Parasitol 34, 3: 275 EOF84 EOF
  59. 59. NowakowskaD.ColonI.RemingtonJ. S.GriggM.GolabE.WilczynskiJ.SibleyL. D.2006Genotyping of Toxoplasma gondii by multiplex PCR and peptide-based serological testing of samples from infants in Poland diagnosed with congenital toxoplasmosis. J Clin Microbiol 44, 4: 1382 EOF9 EOF
  60. 60. OkayT. S.YamamotoL.OliveiraL. C.ManuliE. R.AndradeJunior. H. F.Del NegroG. M.2009Significant performance variation among PCR systems in diagnosing congenital toxoplasmosis in São Paulo, Brazil: analysis of 467 amniotic fluid samples. Clinics (Sao Paulo) 64, 3: 171-6.
  61. 61. OkhraviN.JonesC. D.CarrollN.AdamsonP.LuthertP.LightmanS.2005Use of PCR to diagnose Toxoplasma gondii chorioretinitis in eyes with severe vitritis. Clin Experiment Ophthalmol 33, 2: 184 EOF187 EOF
  62. 62. PrestrudK. W.AsbakkK.MorkT.FugleiE.TrylandM.SuC.2008Direct high-resolution genotyping of Toxoplasma gondii in arctic foxes (Vulpes lagopus) in the remote arctic Svalbard archipelago reveals widespread clonal Type II lineage. Vet Parasitol 158, 1-2: 121 EOF128 EOF
  63. 63. ReischlU.BretagneS.KrugerD.ErnaultP.CostaJ. M.2003Comparison of two DNA targets for the diagnosis of Toxoplasmosis by real-time PCR using fluorescence resonance energy transfer hybridization probes. BMC Infect Dis 3, 7 EOF
  64. 64. RichommeC.AubertD.Gilot-FromontE.AjzenbergD.MercierA.DucrotC.FerteH.DelormeD.VillenaI.2009Genetic characterization of Toxoplasma gondii from wild boar (Sus scrofa) in France. Vet Parasitol 164, 2-4: 296 EOF300 EOF
  65. 65. RomandS.WallonM.FranckJ.ThulliezP.PeyronF.DumonH.2001Prenatal diagnosis using polymerase chain reaction on amniotic fluid for congenital toxoplasmosis. Obstet Gynecol 97, 2: 296 EOF300 EOF
  66. 66. SabajV.GalindoM.SilvaD.SandovalL.RodríguezJ. C.2010Analysis of Toxoplasma gondii surface antigen 2 gene (SAG2). Relevance of genotype I in clinical toxoplasmosis. Mol Biol Rep 37, 6: 2927 EOF2933 EOF
  67. 67. daSilva. R. C.LangoniH.SuC.daSilva. A. V.2011Genotypic characterization of Toxoplasma gondii in sheep from Brazilian slaughterhouses: new atypical genotypes and the clonal type II strain identified. Vet Parasitol 175, 1-2: 173 EOF7 EOF
  68. 68. de CostaJ.DardeM. L.ThulliezP.DubeyJ. P.2006Biologic and molecular characterization of Toxoplasma gondii isolates from pigs from Portugal. Vet Parasitol 135, 2: 133 EOF6 EOF
  69. 69. SuC.EvansD.ColeR. H.KissingerJ. C.AjiokaJ. W.SibleyL. D.2003Recent expansion of Toxoplasma through enhanced oral transmission. Science 299, 5605: 414 EOF6 EOF
  70. 70. SuC.ZhangX.DubeyJ. P.2006Genotyping of Toxoplasma gondii by multilocus PCR-RFLP markers: a high resolution and simple method for identification of parasites. Int J Parasitol 36, 7: 841 EOF848 EOF
  71. 71. SuC.ShwabE. K.ZhouP.ZhuX. Q.DubeyJ. P.1 EOF11 EOF
  72. 72. SwitajK.MasterA.SkrzypczakM.ZaborowskiP.2005Recent trends in molecular diagnostics for Toxoplasma gondii infections. Clin Microbiol Infect 11, 3: 170 EOF176 EOF
  73. 73. TalabaniH.AsserafM.YeraH.DelairE.AncelleT.ThulliezP.BrezinA. P.Dupouy-CametJ.2009Contributions of immunoblotting, real-time PCR, and the Goldmann-Witmer coefficient to diagnosis of atypical toxoplasmic retinochoroiditis. J Clin Microbiol 47, 7: 2131 EOF2135 EOF
  74. 74. TruppelJ. H.ReifurL.Montiani-FerreiraF.LangeR. CastroVilani. R. G.GennariS. M.Thomaz-SoccolV.2010Toxoplasma gondii in Capybara (Hydrochaeris hydrochaeris) antibodies and DNA detected by IFAT and PCR. Parasitol Res 107, 1: 141 EOF146 EOF
  75. 75. ThulliezP.DaffosF.ForestierF.1992Diagnosis of Toxoplasma infection in the pregnant woman and the unborn child: current problems. Scand J Infect Dis Suppl 841822
  76. 76. VidalJ. E.ColomboF. OliveiraA. C.FocacciaR.Pereira-ChioccolaV. L.2004PCR assay using cerebrospinal fluid for diagnosis of cerebral toxoplasmosis in Brazilian AIDS patients. J Clin Microbiol 42, 10: 4765 EOF8 EOF
  77. 77. VillardO.FilisettiD.Roch-DeriesF.GarwegJ.FlamentJ.CandolfiE.2003Comparison of enzyme-linked immunosorbent assay, immunoblotting, and PCR for diagnosis of toxoplasmic chorioretinitis. J Clin Microbiol 41, 8: 3537 EOF41 EOF
  78. 78. VujanićM.2012Molecular detection and genotyping of Toxoplasma gondii strains isolated in Serbia. PhD thesis. University of Belgrade, Serbia.
  79. 79. VujanićM.IvovićV.KataranovskiM.NikolićA.BobićB.KlunI.VillenaI.KataranovskiD.Djurković-DjakovićO.2011Toxoplasmosis in naturally infected rodents in Belgrade, Serbia. Vector Borne Zoonotic Dis 11, 8: 1209 EOF1211 EOF
  80. 80. WahabT.EdvinssonB.PalmD.LindhJ. J.2010Comparison of the AF146527 and B1 repeated elements, two real-time PCR targets used for detection of Toxoplasma gondii. Clin Microbiol 48, 2: 591 EOF592 EOF
  81. 81. WallonM.FranckJ.ThulliezP.HuissoudC.PeyronF.Garcia-MericP.KiefferF.2010Accuracy of real-time polymerase chain reaction for Toxoplasma gondii in amniotic fluid. Obstet Gynecol 115, 4: 727 EOF733 EOF
  82. 82. YeraH.FilisettiD.BastienP.AncelleT.ThulliezP.DelhaesL.2009Multicenter comparative evaluation of five commercial methods for toxoplasma DNA extraction from amniotic fluid. J Clin Microbiol 47, 12: 3881-3886.

Written By

Vladimir Ivovic, Marija Vujanic, Tijana Zivkovic, Ivana Klun and Olgica Djurkovic-Djakovic

Submitted: 05 June 2012 Published: 12 September 2012