Skip to main content

Serosurvey and molecular detection of the main zoonotic parasites carried by commensal Rattus norvegicus population in Tehran, Iran



Rattus norvegicus are reservoirs for transmission of various zoonotic parasites, and they have become a threat to public health worldwide. Given the large number and the significant presence of R. norvegicus throughout the city of Tehran, this study aims to assess the frequency of zoonotic parasites carried by commensal rodents wandering in Tehran, Iran. The study considered the north, south, west, east, and center regions of Tehran for the purposes of this study. The serological tests were applied in order to detect effective antibodies against Trichomonas vaginalis (T. vaginalis), Babesia spp., and Cryptosporidium spp. using a commercial qualitative rat ELISA kit. The frequency of Toxoplasma gondii (T. gondii) was surveyed by using the conventional PCR method. Furthermore, nested PCR was employed to detect the presence of Giardia spp. and Leishmania spp. in commensal R. norvegicus dispersed in Tehran.


Approximately, 76% of the 100 R. norvegicus tested were infected with at least one zoonotic parasite, indicating the significant frequency of parasites within the study areas. Seroreactivity against T. vaginalis, Babesia spp., and Cryptosporidium spp. was detected in 5%, 0%, and 1% of the R. norvegicus tested, respectively. T. gondii DNA was detected in 32 out of 100 (32%) R. norvegicus. In addition, Leishmania spp. and Giardia spp. DNA were found in 18 out of 100 (18%) and 76 out of 100 (76%) R. norvegicus investigated, respectively. T. vaginalis with 15% and T. gondii with 70% had the highest frequency of parasites among the R. norvegicus collected from the western and northeastern regions of Tehran, respectively. Moreover, Giardia spp. with 95% and Leishmania spp. with 30% had the highest frequency in the east and center districts, respectively.


The findings showed a wide geographical dissemination of Giardia spp., Toxoplasma gondii, and Leishmania spp. in R. norvegicus within five districts of Tehran. In contrast, other parasites such as Cryptosporidium spp. infection were rarely detected in Rattus populations. No evidence for the circulation of Babesia spp. was found in this study.


Zoonotic parasites cause a significantly high rate of human infections [1]. It is predicted that 61% of pathogens, which are recognized to have infected individuals, can cause zoonosis [2]. Zoonotic parasites are transmitted between animals and persons with or without vectors; however, eating foods contaminated by rodent feces or urine and inhaling the germ found in feces of rodents are considered the most important pathways for parasite transmission [3,4,5]. Rattus norvegicus globally live and feed in close proximity to human populations and are known to carry various pathogens including bacteria, viruses, and parasites [6]. In urban areas, R. norvegicus represent a reservoir for transmission of zoonotic pathogens, especially zoonotic parasites, and they are linked to various important hygienic problems; they are also responsible for human morbidity and mortality, worldwide [7]. Many of these zoonotic parasites including Leishmania spp., Giardia spp., T. gondii, T. vaginalis, and Cryptosporidium spp. are assumed to be endemic in R. norvegicus populations around the world [8,9,10,11]. Currently, seventy-nine species of rodents have been approximately recognized in Iran; among these previously identified rodents, R. norvegicus are frequently populated in the urban areas as their habitats [12]. Although these rats potentially transmit a large number of zoonotic parasites, the prevalence and diversity of parasites in urban R. norvegicus population remain unknown and the data concerning zoonotic parasites of R. norvegicus are quite insufficient.

Tehran, the capital of Iran, is the largest city in the northern part of Iran that features a continental-influenced hot-summer Mediterranean climate. Home to a population of about 10–12 million in the city and 15 million over the larger metropolitan area of Greater Tehran, Tehran is the most populous city in Iran and Western Asia and ranks as the second largest metropolitan area in the Middle East [13,14,15]. However, the prevalence and diversity of parasites in R. norvegicus populations in Tehran remain unknown, and a comprehensive parasitological assessment of R. norvegicus populations has not been conducted so far.

Therefore, the present study conducts a survey of the R. norvegicus collected from five districts of Tehran for the main zoonotic parasites. The survey provides the first informative data on the traces of zoonotic parasites existing in R. norvegicus in the urban areas of Tehran, Iran.


Detection of Trichomonas vaginalis, Babesia spp., and Cryptosporidium spp.

A total of 100 live Rattus norvegicus (20 rats from each district of Tehran) were captured and surveyed in order to determine their zoonotic parasites (Fig. 1).

Fig. 1
figure 1

A schematic map of the region sampling was done and the frequency of each surveyed parasites among the Rattus population in Tehran, Iran

Males (n = 80) were trapped more often than females (n = 20). The distribution of surveyed parasites among male and female R. norvegicus is shown in Table 1.

Table 1 The frequency of surveyed parasites among male and female Rattus

To detect T. vaginalis, Babesia spp., and Cryptosporidium spp. in the trapped rats, the presence of rat IgG antibodies was examined by ELISA kit. In total, results of serological assay revealed that of the 100 rats captured in Tehran, 5% (n = 5/100) and 1% (n = 1/100) were positive for T. vaginalis and Cryptosporidium spp., respectively. Among the five different districts, T. vaginalis had the highest frequency (15%, n = 3/20) among the R. norvegicus collected from the western part of Tehran. However, this parasite was not detected in the northern and central parts of Tehran. On the other hand, Cryptosporidium spp. was detected only in one rat, collected from the central part of Tehran. Babesia spp. was not detected in any of the 100 serum samples of all 100 animals examined.

Detection of T. gondii, Giardia spp., and Leishmania spp.

In this study, the PCR method was employed to screen the presence of T. gondii in the fecal samples collected from R. norvegicus. Moreover, nested PCR was used to detect Giardia spp. and Leishmania spp. using specific primer pairs. Table 2 shows the number of R. norvegicus and sample types positive for zoonotic parasites in five districts of Tehran. Results showed that the percentage of the animals tested positive for T. gondii in the five regions of Tehran was 32%. Among R. norvegicus trapped in Tehran, T. gondii was of the highest and lowest frequencies in the north (70%, n = 14/20) and west (5%, n = 1/20) districts, respectively. Leishmania spp. molecular analysis of serum samples resulted in the detection of 18 out of 100 (18%) samples, originating from northern (15%, n = 3/20), southern (15%, n = 3/20), eastern (15%, n = 3/20), western (15%, n = 3/20), and central (30%, n = 6/20) parts of Tehran. Giardia spp. was of the highest frequency among the surveyed parasites. In general, according to the results of nested PCR assay, of the 100 rats captured in Tehran, 76% (n = 76/100) were positive for Giardia spp., originating from eastern (95%, n = 19/20), central (80%, n = 16/20), southern (75%, n = 15/20), western (65%, n = 13/20), and northern (65%, n = 13/20) parts of Tehran.

Table 2 Numbers of Rattus norvegicus and sample types positive for zoonotic parasites identified in five districts of Tehran


In general, in urban areas, rodents such as Rattus norvegicus exist in large populations and represent a significant reservoir of different human pathogens including bacteria, viruses, and parasites [6, 16]. The results revealed that Giardia spp. was the main parasite that was frequently (76%; n = 76/100) isolated from the Rattus population of Tehran. In addition, the frequency of Giardia spp. was quite high in the eastern (95%, n = 19/20) part of Tehran. This finding illustrates that Giardia spp. is the main gastrointestinal parasite in the Rattus population and these rodents are the reservoir of this parasite. Moreover, this result shows that rats can transmit Giardia spp. to humans and cause severe infections such as giardiasis [17]. Therefore, a number of more effective measures such as appropriate maintenance of hygienic conditions, regular disinfection of urban environments (dumping garbage sites, the open water canal, and gardens), and prevention of the contamination of food and water sources against Giardia spp. need to be taken by the government and healthcare workers to combat zoonosis. Obtained results are in agreement with those of previous studies from Germany [17], Grenada [18], and Poland (two studies) [18, 19], which reported that the prevalence of Giardia spp. among rodents was 73%, 55%, 50%, and 70%, respectively. These studies stated that rodents were the significant reservoirs of Giardia spp. However, this result is not consistent with those of published studies by Chagas et al. in Brazil [20], Perec-Matysiak et al. in Poland [21], and Li et al. in USA [22]. These three studies found that the frequency of Giardia spp. in the rodent population was 42.9%, < 35%, and 24.2%, respectively.

The result of our study revealed that T. gondii had the highest frequency (70%; n = 14/20) in the Rattus captured from the northern part of Tehran. The total frequency of T. gondii was 32%. Globally, T. gondii is a common zoonosis which is considered as an obligate intracellular parasite and causes toxoplasmosis [23]. Cats are the main source of toxoplasma eggs and are the definitive hosts that shed eggs (oocysts) in feces. Rats serve as intermediate hosts of T. gondii, and the ingestion of toxoplasma oocysts is the most common way individuals contract toxoplasmosis [24]. It is revealed that naturally infected rodents can act as significant reservoir hosts and have a critical role in spreading T. gondii to other animals including pigs, dogs, and cats [23]. Our findings are comparable with those of Dellarupe et al. from Argentina [25], Yan et al. from China [23], Ahmad et al. from Pakistan [26], Mosallanejad et al. from Iran [27], and Salibay et al. from the Philippines [28]. These studies found that the frequency of T. gondii in the rodent population was 32.8%, 23.9%, 11 to 58%, 24.41%, and 58%, respectively. However, Pellizzaro et al. from Brazil [8], Saki et al. from Ahvaz district of Iran [10], Gennari from Brazil [9], and Yin from China [29] showed that the frequency of T. gondii in Rattus population was 4.6%, 6%, 8.6%, and 3.2%, respectively. The relatively high frequency of T. gondii in rodents suggests that rodents are possibly one of the important reservoirs of this parasite. However, the percent frequency of T. gondii infection varies between geographical areas and is dissimilar in different parts of the world. The prevalence of toxoplasma infection can be affected by a number of factors such as (a) close association with the wild and domestic animals acting as definitive and intermediate hosts; (b) different hygienic conditions of countries; (c) different awareness levels, educational status, and poverty; and (d) differences in population structure and feeding habits among different countries around the world [26]. Generally, the high frequency of Giardia spp. and T. gondii in the Rattus population in Tehran is an important concern. Therefore, sanitary control is extremely important to observe in Tehran. Moreover, these data assist veterinarians and physicians with better diagnostic and preventative measures.

The frequency of Leishmania-positive Rattus population was 18% lower than what has been found in other studies. For example, Motazedian et al. detected Leishmania major (52%) in the Rattus population in Iran [30]. Akhoundi et al. found Leishmania spp. (31.4%) in the rodent population in Iran [31]. Navea-Pérez et al. detected Leishmania infantum (27%) in the trapped rodents in Spain [32]. Marcelino et al. identified Leishmania (36.25%) in the Rattus population in Brazil [33]. Dohlen et al. confirmed the existence of Leishmania (23.3%) in the Rattus population in the USA [34]. Tsakmakidis et al. detected high frequency of Leishmania (70%) in the R. norvegicus population in Greece [35].

The small number of positive cases in the current study in comparison to other studies is justified through reasons such as type of sample and methods used to detect Leishmania spp. and the different hygienic levels of countries. However, our results were consistent with the findings of several studies conducted by Echchakery et al. from Morocco [36], Marcelino et al. from Brazil [33], Davami et al. from Iran [37], and Pereira et al. from Brazil [38]. They revealed that the frequency of Leishmania spp. in the rodent population was 11.1%, 17.46%, 14.6%, and 20%, respectively. Leishmaniasis is a vector-borne infectious disease and is considered to be a major public health problem in the urban environment. The diagnosis of natural hosts of Leishmania spp. in urban areas is a necessity, which will facilitate a better understanding of the epidemiology of the leishmaniasis [39].

The prevalence of Cryptosporidium spp. among Rattus population was 1% lower than what was found by other studies around the world. The findings of other studies conducted in the four above-mentioned countries revealed that the prevalence rate of Cryptosporidium spp. in the rodent population was 38% [40], > 60% [21], 34.2% [41], and 25.8% [42], respectively. However, the results of several other related studies were relatively consistent with our findings, and they reported that the frequency of Cryptosporidium spp. in the rodent population was < 10% [43,44,45]. According to the reports, it is concluded that rodent population can act as a potential reservoir of Cryptosporidium spp. and probably transmit this important enteric pathogen to humans.

This study applied the commercial qualitative rat ELISA kit to the screening of antibodies against T. vaginalis among Rattus serum samples. Our findings revealed that the prevalence of T. vaginalis among the Rattus population was 5%. As far as we are concerned, the present study is the first research to have investigated the prevalence of T. vaginalis in the Rattus population, worldwide.


The finding of our study indicates that the Rattus norvegicus population is a significant reservoir of Giardia spp., T. gondii, and Leishmania spp. infections for humans in Tehran. It is important to raise public attention to and awareness of the transmission risk of contracting these diseases through the Rattus population. Information about zoonotic parasites carried by the R. norvegicus population in Tehran province is critical to developing suitable surveillance plans and intervention strategies.


Site selection and sample collection

This study concentrated on five regions (north, south, west, east, and center) of Tehran. Alleys behind the residential dwellings in urban areas were the trapping locations. A sampling strategy was designed to trap 20 rats in each region between October 2018 and June 2019. Rodent sampling was carried out by using Sherman live traps and alluring baits through convenient sampling method. Rats were found mostly around dumping garbage sites along open water canals and gardens as their aggregated habitats. Given that the Tehran Municipality takes physical and chemical measures to control rats, catching rodents has become challenging and problematic; therefore, a prebaiting procedure is preferable for improving the efficiency of traps. Trapping was set after sundown in each selected region and processed during midnight or the next morning. Traps were distributed in order to manage the present situation. Collected rodents were transferred to a guaranteed special laboratory in animal houses, and then, they were euthanized by the intramuscular injection of ketamine and xylazine (0.1 mg/kg) followed by bilateral thoracotomy. Finally, fecal samples were collected, and blood samples were obtained via cardiac puncture using a 5-mL syringe; then, the serum was recovered after centrifugation and stored at − 80 °C prior to serological analysis. The subsequent parasitological examination was conducted at the Department of Microbiology of Shahid Beheshti University of Medical Sciences.

Enzyme-linked immunosorbent assay

Serum samples were screened for antibodies against T. vaginalis, Babesia spp., and Cryptosporidium spp. by using commercial qualitative rat enzyme-linked immunosorbent assay (ELISA) kit (Shanghai Crystal day Biotech Co., Ltd) according to the manufacturer’s instructions. The optical density (OD value) of each well was measured by immediately using a microplate reader set at 450 nm (OD450) within 15 min after adding the stop solution (sulfuric acid).

DNA extraction and polymerase chain reaction

Genomic DNA was extracted from fecal samples using the DNA extraction kit (AllPrep DNA minikit (Qiagen, Inc.) according to the manufacturer’s guidelines, and each DNA sample was eluted in 200 ml buffer preserved at − 80 °C until further use. Polymerase chain reaction (PCR) was conducted to detect T. gondii using specific primer pairs including F: 5′-GTAGCGTGCTTGTTGGCGAC-3′ and R: 5′-ACAAGACATAGAGTGCCCC-3′.

PCR was conducted at a final volume of 25 μl including 0.5 μl of 10 mM of each deoxynucleoside triphosphate (dNTPs), 3 μl of 10× PCR buffer without MgCl2, 2.5 mmol/l MgCl2, 1 unit of Taq polymerase (Cinnagene, Iran), 0.5 μM of each primer (10 mM), 3 μl of template DNA, and 7.5 μL of sterile distilled water. Amplification reactions were performed under the following condition: one cycle at 95 °C for 4 min, followed by 36 cycles at 94 °C for 45 s, annealing at 56 °C for 45 s, and preservation at 72 °C for 1 min with the final extension step at 72 °C for 10 min following the last cycle. PCR products were screened on a 1–1.5% agarose gel, visualized by DNA safe stain (SinaClon Co., Iran), and photographed under UV light. Moreover, PCR-amplified products were confirmed by sequencing analysis (Macrogen Korea), and the obtained sequence results were examined by using the NCBI BLAST program (Primer blast).

Nested PCR

Nested PCR was used for detecting Giardia spp. and Leishmania spp. using specific primer pairs. In brief, Leishmania DNA was amplified and detected using the first-round primer pairs including 5′-CTGGATCATTTTCCGATG-3′ and 5′-TGATACCACTTATCGCACTT-3′ and the second-round primers including 5′-CATTTTCCGATGATTACACC-3′ and 5′-CGTTCTTCAACGAAATAGG-3′. PCR conditions at the first step were set based on a previously published study by Salotra et al. [46]. Giardia spp. DNA was amplified using the first-round primer pairs including G7-F: 5′-AAGCCCGACGACCTCACCCGCAGTGC-3′ and G759-R: 5′-GAGGCCGCCCTGGATCTTCGAGACGAC-3′ and the second round primers including BG1-F: 5′-GAACGAGATCGAGGTCCG-3′ and BG2-R: 5′-CTCGACGAGTTCGTGTT-3′. PCR conditions at the first step were set based on a previously published study by Ayan et al. [47]. In summary, PCR was conducted with the final volume of 50 μl including 10 mM Tris-HCl (pH 8.3) and 50 mM KCl, a 200-μM concentration of each dNTP, 1.5 mM MgCl2, 1.25 U of Taq DNA polymerase (Invitrogen), 50 ng of each primer, 5 μl DNA, and 1× PCR buffer (Invitrogen). For the second round, the method provided by Sreenivas et al. was used [48]. Briefly, the second round was performed with a total volume of 50 μl containing 10 mM Tris-HCl (pH 8.3), 50 mM KCl, 200 mM of each dNTP, 1.5 mM MgCl2, 2 mM of each primer, and 1.5 U platinum Taq DNA polymerase (Invitrogen). Moreover, we used 1 μl of the diluted (1:10) products from the first-round reaction as a template. Amplification reactions were performed under the following condition: initial denaturation at 94 °C for 5 min followed by 35 cycles at 94 °C for 1 min, annealing at 50–54 °C for 1 min, and preservation at 72 °C for 90 s with the final extension at 72 °C for 3 min. PCR products were screened on a 1% agarose gel, visualized by DNA safe stain (SinaClon Co., Iran), and photographed under UV light; they were confirmed by sequencing analysis (Macrogen Korea). The sequencing results were examined by the NCBI BLAST program (Primer blast).

Statistical analysis

The data were formatted in an SPSS file, and the frequency of each surveyed parasite was analyzed by the statistical package SPSS v.23.0 (SPSS Inc., Chicago, IL, USA) using descriptive statistic tests.

Availability of data and materials

All data generated or analyzed during this study are included in this published article.


R. norvegicus :

Rattus norvegicus

T. vaginalis :

Trichomonas vaginalis

T. gondii :

Toxoplasma gondii


Polymerase chain reaction


Enzyme-linked immunosorbent assay


Optical density


Deoxynucleoside triphosphate


  1. Galán-Puchades MT, Sanxis-Furió J, Pascual J, Bueno-Marí R, Franco S, Peracho V, et al. First survey on zoonotic helminthosis in urban brown rats (Rattus norvegicus) in Spain and associated public health considerations. Vet Parasitol. 2018;259:49–52.

    PubMed  Google Scholar 

  2. Cantas L, Suer K. The important bacterial zoonoses in “one health” concept. Front Public Health. 2014;2:144.

    PubMed  PubMed Central  Google Scholar 

  3. Meerburg BG, Singleton GR, Kijlstra A. Rodent-borne diseases and their risks for public health. Crit Rev Microbiol. 2009;35(3):221–70.

    PubMed  Google Scholar 

  4. Guenther S, Bethe A, Fruth A, Semmler T, Ulrich RG, Wieler LH, et al. Frequent combination of antimicrobial multiresistance and extraintestinal pathogenicity in Escherichia coli isolates from urban rats (Rattus norvegicus) in Berlin, Germany. PLoS One. 2012;7(11):e50331.

    CAS  PubMed  PubMed Central  Google Scholar 

  5. Maas M, De Vries A, Reusken C, Buijs J, Goris M, Hartskeerl R, et al. Prevalence of Leptospira spp. and Seoul hantavirus in brown rats (Rattus norvegicus) in four regions in the Netherlands, 2011-2015. Infect Ecol Epidemiol. 2018;8(1):1490135.

    PubMed  PubMed Central  Google Scholar 

  6. Firth C, Bhat M, Firth MA, Williams SH, Frye MJ, Simmonds P, et al. Detection of zoonotic pathogens and characterization of novel viruses carried by commensal Rattus norvegicus in New York City. mBio. 2014;5(5):e01933-e01914.

  7. Himsworth CG, Bai Y, Kosoy MY, Wood H, DiBernardo A, Lindsay R, et al. An investigation of Bartonella spp., Rickettsia typhi, and Seoul hantavirus in rats (Rattus spp.) from an inner-city neighborhood of Vancouver, Canada: is pathogen presence a reflection of global and local rat population structure? Vector Borne Zoonotic. 2015;15(1):21–6.

    Google Scholar 

  8. Pellizzaro M, FdO C, Martins CM, Joaquim SF, Ferreira F, Langoni H, et al. Serosurvey of Leptospira spp. and Toxoplasma gondii in rats captured from two zoos in Southern Brazil. Rev Soc Bras Med Trop. 2017;50(6):857–60.

    PubMed  Google Scholar 

  9. Gennari SM, Ogrzewalska MH, Soares HS, Saraiva DG, Pinter A, Nieri-Bastos FA, et al. Toxoplasma gondii antibodies in wild rodents and marsupials from the Atlantic Forest, state of São Paulo, Brazil. Rev Bras Parasitol Vet. 2015;24(3):379–82.

    CAS  PubMed  Google Scholar 

  10. Saki J, Khademvatan S. Detection of Toxoplasma gondii by PCR and mouse bioassay in rodents of Ahvaz District, Southwestern Iran. Biomed Res Int. 2014;2014.

  11. Murata FH, Cerqueira-Cézar CK, Kwok OC, Tiwari K, Sharma RN, Su C, et al. Role of rats (Rattus norvegicus) in the epidemiology of Toxoplasma gondii infection in Grenada, West Indies. J Parasitol. 2018;104(5):571–3.

    CAS  PubMed  Google Scholar 

  12. Rabiee MH, Mahmoudi A, Siahsarvie R, Kryštufek B, Mostafavi E. Rodent-borne diseases and their public health importance in Iran. PLoS Negl Trop Dis. 2018;12(4):e0006256.

    PubMed  PubMed Central  Google Scholar 

  13. Azimi T, Nasiri MJ, Zamani S, Hashemi A, Goudarzi H, Fooladi AAI, et al. High genetic diversity among Mycobacterium tuberculosis strains in Tehran, Iran. J Clin Tuberc Other Mycobact Dis. 2018;11:1–6.

    PubMed  PubMed Central  Google Scholar 

  14. Azimi T, Shariati A, Fallah F, Imani Fooladi AA, Hashemi A, Goudarzi H, et al. Mycobacterium tuberculosis genotyping using MIRU-VNTR typing. Majallahi Danishgahi Ulumi Pizishkii Mazandaran. 2017;27(149):40–8.

    Google Scholar 

  15. Sharifipour S, Rad KDJ. Seroprevalence of hepatitis E virus among different age groups in Tehran, Iran. New Microbes New Infect. 2019;34:100638.

    PubMed  PubMed Central  Google Scholar 

  16. Himsworth CG, Feng AY, Parsons K, Kerr T, Patrick D. Using experiential knowledge to understand urban rat ecology: a survey of Canadian pest control professionals. Urban Ecosyst. 2013;16(2):341–50.

    Google Scholar 

  17. Helmy YA, Spierling NG, Schmidt S, Rosenfeld UM, Reil D, Imholt C, et al. Occurrence and distribution of Giardia species in wild rodents in Germany. Parasit Vectors. 2018;11(1):213.

    PubMed  PubMed Central  Google Scholar 

  18. Tiwari K, Springer CC, Chikweto A, Tang J, Sepulveda Y, Smith AL, et al. Giardiasis: serum antibodies and coproantigens in brown rats (Rattus norvegicus) from Grenada, West Indies. Vet World. 2018;11(3):293.

    PubMed  PubMed Central  Google Scholar 

  19. Bajer AJ. Between-year variation and spatial dynamics of Cryptosporidium spp. and Giardia spp. infections in naturally infected rodent populations. Parasitology. 2008;135(14):1629–49.

    CAS  PubMed  Google Scholar 

  20. Chagas CRF, Gonzalez IHL, Favoretto SM, Ramos PLJ. Parasitological surveillance in a rat (Rattus norvegicus) colony in São Paulo Zoo animal house. Ann Parasitol. 2017;63(4):291–7.

    PubMed  Google Scholar 

  21. Perec-Matysiak A, Bunkowska-Gawlik K, Zalesny G, Hildebrand JJ. Small rodents as reservoirs of Cryptosporidium spp. and Giardia spp. in south-western Poland. Ann Agric Environ Med. 2015;22(1).

  22. Li X, Atwill ER, Vivas E, Vodovoz T, Xiao C, Jay-Russell M. Detection and prevalence of Cryptosporidium spp. and Giardia spp. from wild rodents adjacent to produce production fields in California. Proc Vertebrate Pest Conf. 2012.

  23. Yan C, Liang L-J, Zhang B-B, Lou Z-L, Zhang H-F, Shen X, et al. Prevalence and genotyping of Toxoplasma gondii in naturally-infected synanthropic rats (Rattus norvegicus) and mice (Mus musculus) in eastern China. Parasit Vectors. 2014;7(1):591.

    PubMed  PubMed Central  Google Scholar 

  24. Araújo JB, da Silva AV, Rosa RC, Mattei RJ, da Silva RC, Richini-Pereira VB, et al. Isolation and multilocus genotyping of Toxoplasma gondii in seronegative rodents in Brazil. Vet Parasitol. 2010;174(3-4):328–31.

    PubMed  Google Scholar 

  25. Dellarupe A, Fitte B, Pardini L, Campero LM, Bernstein M, Robles MR, et al. Toxoplasma gondii and Neospora caninum infections in synanthropic rodents from Argentina. Braz J Vet Pathol. 2019;28(1):113–8.

    CAS  Google Scholar 

  26. Ahmad M, Maqbool A, Mahmood-ul-Hassan M, Mushtaq-ul-Hassan M, Anjum AJ. Prevalence of Toxoplasma gondii antibodies in human beings and commensal rodents trapped from Lahore, Pakistan. J Anim Plant Sci. 2012;22:51–3.

    Google Scholar 

  27. Mosallanejad B, Avizeh R, Razi JMH, Hamidinejat H. Seroprevalence of Toxoplasma gondii among wild rats (Rattus rattus) in Ahvaz District, Southwestern Iran. Jundishapur J Microbiol. 2012;5(1):332–5.

    Google Scholar 

  28. Salibay CC, Claveria FG JSAjotm, health p. Serologic detection of Toxoplasma gondii infection in Rattus spp collected from three different sites in Dasmarinas, Cavite, Philippines. Southeast Asian J Trop Med Public Health (Suppl. 4).2005;36: 46-9.

  29. Yin C-C, He Y, Zhou D-H, Yan C, He X-H, Wu S-M, et al. Seroprevalence of Toxoplasma gondii in rats in southern China. J Parasitol. 2010;96(6):1233–5.

    PubMed  Google Scholar 

  30. Motazedian MH, Parhizkari M, Mehrabani D, Hatam G, Asgari Q. First detection of Leishmania major in Rattus norvegicus from Fars province, southern Iran. Vector Borne Zoonotic. 2010;10(10):969–75.

    Google Scholar 

  31. Akhoundi M, Mohebali M, Asadi M, Mahmodi MR, Amraei K, Mirzaei A. Molecular characterization of Leishmania spp. in reservoir hosts in endemic foci of zoonotic cutaneous leishmaniasis in Iran. Folia Parasitol. 2013;60(3):218–24.

    CAS  PubMed  Google Scholar 

  32. Navea-Pérez H, Díaz-Sáez V, Corpas-López V, Merino-Espinosa G, Morillas-Márquez F, Martín-Sánchez J. Leishmania infantum in wild rodents: reservoirs or just irrelevant incidental hosts? Parasitol Res. 2015;114(6):2363–70.

    PubMed  Google Scholar 

  33. Marcelino AP, Ferreira EC, Avendanha JS, Costa CF, Chiarelli D, Almeida G, et al. Molecular detection of Leishmania braziliensis in Rattus norvegicus in an area endemic for cutaneous leishmaniasis in Brazil. Vet Parasitol. 2011;183(1-2):54–8.

    CAS  PubMed  Google Scholar 

  34. von Dohlen AR, Cheathem N, Tiwari K, Sharma R. Prevalence of antibodies against visceralizing Leishmania spp. in brown rats from Grenada, West Indies. Vet World. 2018;11(9):1321–5.

    Google Scholar 

  35. Tsakmakidis Ι, Angelopoulou K, Dovas CI, Dokianakis Ε, Tamvakis Α, Symeonidou I, et al. Leishmania infection in rodents in Greece. Tropical Med Int Health. 2017;22(12):1523–32.

    CAS  Google Scholar 

  36. Echchakery M, Chicharro C, Boussaa S, Nieto J, Carrillo E, Sheila O, et al. Molecular detection of Leishmania infantum and Leishmania tropica in rodent species from endemic cutaneous leishmaniasis areas in Morocco. Parasit Vectors. 2017;10(1):454.

    PubMed  PubMed Central  Google Scholar 

  37. Davami MH, Motazedian MH, Kalantari M, Asgari Q, Mohammadpour I, Sotoodeh-Jahromi A, et al. Molecular survey on detection of Leishmania infection in rodent reservoirs in Jahrom District, Southern Iran, J Arthropod Borne Dis 2014;8(2):139-146.

  38. Pereira AAS, de Castro Ferreira E, da Rocha A. Detection of Leishmania spp. in silvatic mammals and isolation of Leishmania (Viannia) braziliensis from Rattus rattus in an endemic area for leishmaniasis in Minas Gerais State, Brazil. PLoS One. 2017;12(11):e0187704.

    PubMed  PubMed Central  Google Scholar 

  39. Eder M, Cortes F, de Siqueira Filha NT, de França GVA, Degroote S, Braga C, et al. Scoping review on vector-borne diseases in urban areas: transmission dynamics, vectorial capacity and co-infection. Infect Dis Poverty. 2018;7(1):90.

    PubMed  PubMed Central  Google Scholar 

  40. Kimura A, Edagawa A, Okada K, Takimoto A, Yonesho S, Karanis PJ. Detection and genotyping of Cryptosporidium from brown rats (Rattus norvegicus) captured in an urban area of Japan. Parasitol Res. 2007;100(6):1417–20.

    PubMed  Google Scholar 

  41. Song J, Kim C-Y, Chang S-N, Abdelkader TS, Han J, Kim T-H, et al. Detection and molecular characterization of Cryptosporidium spp. from wild rodents and insectivores in South Korea. Korean J Parasitol. 2015;53(6):737–43.

    CAS  PubMed  PubMed Central  Google Scholar 

  42. Ng-Hublin JS, Singleton GR, Ryan UJ. Molecular characterization of Cryptosporidium spp. from wild rats and mice from rural communities in the Philippines. Infect Genet Evol. 2013;16:5–12.

    CAS  PubMed  Google Scholar 

  43. Zhao W, Wang J, Ren G, Yang Z, Yang F, Zhang W, et al. Molecular characterizations of Cryptosporidium spp. and Enterocytozoon bieneusi in brown rats (Rattus norvegicus) from Heilongjiang Province, China. Parasit Vectors. 2018;11(1):313.

    PubMed  PubMed Central  Google Scholar 

  44. Saki J, Foroutan-Rad M, Asadpouri RJ. Molecular characterization of Cryptosporidium spp. in wild rodents of southwestern Iran using 18S rRNA gene nested-PCR-RFLP and sequencing techniques. J Trop Med. 2016;(2):1–6.

  45. Paparini A, Jackson B, Ward S, Young S, Ryan UM. Multiple Cryptosporidium genotypes detected in wild black rats (Rattus rattus) from northern Australia. Exp Parasitol. 2012;131(4):404–12.

    PubMed  Google Scholar 

  46. Salotra P, Sreenivas G, Pogue GP, Lee N, Nakhasi HL, Ramesh V, et al. Development of a species-specific PCR assay for detection of Leishmania donovani in clinical samples from patients with kala-azar and post-kala-azar dermal leishmaniasis. J Clin Microbiol. 2001;39(3):849–54.

    CAS  PubMed  PubMed Central  Google Scholar 

  47. Ayan A, Ural DA, Erdogan H, Kilinc OO, Gültekin M, Ural K. Prevalance and molecular characterization of Giardia duodenalis in livestock in Van, Turkey. Int J Ecosyst Ecol Sci. 2019;9(2):289–96.

    Google Scholar 

  48. Sreenivas G, Ansari N, Kataria J, Salotra P. Nested PCR assay for detection of Leishmania donovani in slit aspirates from post-kala-azar dermal leishmaniasis lesions. J Clin Microbiol. 2004;42(4):1777–8.

    CAS  PubMed  PubMed Central  Google Scholar 

Download references


We would like to thank the “Pediatric Infections Research Center, Shahid Beheshti University of Medical Sciences, Tehran, Iran” for their kind cooperation.


The research reported in this publication was supported by the Elite Researcher Grant Committee under award no. [962763] from the National Institutes for Medical Research Development (NIMAD), Tehran, Iran.

Author information

Authors and Affiliations



Taher Azimi and Mohammad Reza Pourmand: conceptualization, data curation, formal analysis, and writing—original draft. Fatemeh Fallah, Abdollah Karimi, and Lela Azimi: conceptualization, methodology, project administration, and writing—original draft. Roxana Mansour-Ghanaie, Mehdi Shirdoust, and Seyedeh Mahsan Hoseini-Alfatemi: data curation, formal analysis, writing—original draft, and writing—review and editing. Taher Azimi and Leila Azimi: language editing. The author(s) read and approved the final manuscript.

Corresponding author

Correspondence to Leila Azimi.

Ethics declarations

Ethics approval and consent to participate

The present study was approved by the Ethics Committee of National Institutes for Medical Research Development (NIMAD) with reference number IR.NIMAD.REC. 1396.323.

Consent for publication

All authors made substantial contributions to the conception and design, acquisition of data, or analysis and interpretation of data. They played an active role in drafting the article or revising it critically to achieve important intellectual content, gave the final approval of the version to be published, and agreed to be accountable for all aspects of the work.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Azimi, T., Pourmand, M.R., Fallah, F. et al. Serosurvey and molecular detection of the main zoonotic parasites carried by commensal Rattus norvegicus population in Tehran, Iran. Trop Med Health 48, 60 (2020).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: