Toxoplasmosis seroprevalence in urban rodents: a survey in Niamey, Niger

Abstract

A serological survey of Toxoplasma gondii was conducted on 766 domestic and peridomestic rodents from 46 trapping sites throughout the city of Niamey, Niger. A low seroprevalence was found over the whole town with only 1.96% of the rodents found seropositive. However, differences between species were important, ranging from less than 2% in truly commensal Mastomys natalensis, Rattus rattus and Mus musculus, while garden-associated Arvicanthis niloticus displayed 9.1% of seropositive individuals. This is in line with previous studies on tropical rodents - that we reviewed here - which altogether show that Toxoplasma seroprevalence in rodent is highly variable, depending on many factors such as locality and/or species. Moreover, although we were not able to decipher statistically between habitat or species effect, such a contrast between Nile grass rats and the other rodent species points towards a potentially important role of environmental toxoplasmic infection. This would deserve to be further scrutinised since intra-city irrigated cultures are extending in Niamey, thus potentially increasing Toxoplasma circulation in this yet semi-arid region. As far as we are aware of, our study is one of the rare surveys of its kind performed in Sub-Saharan Africa and the first one ever conducted in the Sahel.

Toxoplasma gondii; epidemiology; zoonotic disease; Africa; Sahel

Sahel is a sub-arid region that undergoes rapid climatic changes (Lebel & Ali 2009) with dramatic consequences on food production and availability. Such a critical situation leads to a massive rural exodus and extensive urbanisation. Niamey, the main town of Niger, is no exception. Since the 1960s, the population of this rather young city has been undergoing an explosive increase due to a very important demographic growth (Sidikou 2011). The number of inhabitants has increased from ~3,000 in the 1920s, > 30,000 in the late 1950s to 707,000 in 2001 and reached more than 1.2 million in 2010 (Sidikou 2011, Adamou 2012). As often in such cases, this was accompanied by many informal settlements and insufficient tracking of necessary sanitary services.

Along with other problems, public health is a primordial concern with low clinical capacities and poor accessibility to medical care. In addition, robust epidemiological data for Niger remains scarce for many major diseases such as malaria and human immunodeficiency virus (HIV). From there, other pathologies are even more poorly documented, when not undetected, due to weak screening programs and/or diagnostic facilities. Among them, the worldwide distributed toxoplasmosis is induced by the intracellular protozoan Toxoplasma gondii whose infection may be asymptomatic to lethal, with primo-infection being particularly dangerous during pregnancy due to subsequent abortion or severe clinical consequences on foetus and neonate. Moreover, toxoplasmosis appears as an opportunistic disease in immuno-depressed patients such as HIV-positive ones (Robert-Gangneux & Dardé 2012).

In sub-Saharan Africa, human prevalence [reviewed in Mercier (2010) ] ranges from 3.9% in Niger (Delacroix & Laporte 1989) to 83.5% in Madagascar (Lelong et al. 1995). In Niger, toxoplasmosis has only been the focus of five studies and seroprevalence values were found to be quite variable, ranging from 3.9-50.5%, with an average of 12.8% for the whole country (Table I). A survey conducted on 218 pregnant women in Niamey showed a slightly higher value (i.e. 15.1%) and the most recent survey for the city indicated a global seroprevalence of 18.1% (Table I). On this basis, previous authors have considered toxoplasmosis not to be of primary importance for public health in Niger. Medical monitoring of pregnancy is still poor - when not null - for many women, thus making robust statistics difficult to obtain. Perinatal outcomes, including spontaneous abortion and stillbirth children, seem not to be rare in Niger: the National Service for Sanitary Information (SNIS) evaluate stillborn children to reach 8% (SNIS 2010). In 2010, 37% of patient admissions in the reference maternity hospital in Niamey concerned "abortions" (SNIS 2010). However, such statistics need to be handled with great care since many - if not most - of these cases may be due to complications following illegal abortions (voluntary termination is prohibited in Niger). Such a large proportion of perinatal complications may cast doubt on our perception of the real incidence of the disease in the country. We are aware of no systematic and large-scale monitoring of the disease that would allow one to robustly address the respective role of toxoplasmosis.

TABLE I
Recapitulation of studies conducted in Niger and dealing with Toxoplasma seroprevalence in human

			Raw seroprevalence
References	Geographic level	Target population	NIT	(%)
Dumas et al. (1985)	NA	Infants	14	42.9
		Their mother	14	58.1
Develoux et al. (1988)	Niamey and surroundings	General population	400	18.2
		Urban population	199	11.5
		Rural population	201	24.8
Develoux et al. (1989)	Niamey	Pregnant women	218	15.1
Delacroix & Laporte (1989)	Akokan (Arlit)	Women of reproductive age	229	3.9
Dumas et al. (1991)	Arlit	Pregnant women	242	5.4
		Infants	77	2.6
Julvez et al. (1996)	Niamey and surroundings	General population	371	18

• NA: not available; NIT: number of individuals tested for toxoplasmosis.

Transmission to human and warm-blooded animals occurs via three primary ways, congenitally, by ingestion of food and water contaminated with oocysts shed into the environment in faeces of felids (domestic cat or wild felids) or by the ingestion of undercooked meat containing tissue cysts. Although felids are the only known definitive host, T. gondii may infect all homoeotherm animals (i.e. birds and mammals), which then act as intermediate hosts (Tenter et al. 2000). Among them, rodents are found in most types of terrestrial biotopes, where they constitute important prey for wild as well as domestic felids. Moreover, they are usually among the last wild mammals to persist in highly human-modified environments, like large towns. For these reasons, rodents most probably play a pivotal role in the maintenance and circulation of T. gondii in urban habitats (Dubey & Frenkel 1998, Murphy et al. 2008). A study conducted in the city of Lyon, France, suggested that low Toxoplasma prevalence in stray cats may be in part associated with low rodent densities (Afonso et al. 2006). Surprisingly, however, epidemiological surveys of T. gondii in rodents are scarce, especially those dealing with tropical regions (^{Supplementary data}). Seroprevalences were found to be highly variable depending on the species and/or the region. In Sub-Saharan Africa, where only two studies were conducted (^{Supplementary data}), 100% of seropositive Thryonomys swinderianus individuals (n = 104) were found in South Western Nigeria, while only 2.7% and 2.3% of positive wild and commensal rodents were detected in Gabon (n = 37 and 43, respectively) (^{Supplementary data}). To our knowledge, no such survey has ever been conducted in Sahelian countries.

Recently, human-mediated transport of invasive rodents has been shown to be responsible for the import of allochtonous human pathogens (Dobigny et al. 2011). This motivated a long-term program that aimed to investigate rodents and rodent-borne human pathogens in the city of Niamey. As part of this wider project, we here provide serological results for Toxoplasma that were obtained from 766 rodents. Seroprevalence data are then discussed in regard to native and invasive rodent host species distribution, as well as urban environments in terms of transmission risk to human populations.

MATERIALS AND METHODS

Sampling and species-specific identifications of rodents - From 2009-2011, a multi-approach monitoring of urban rodents was performed in order to address several issues including epidemiological ones. To do so, more than 14,560 night-traps were performed using both Sherman and locally made wire-mesh traps in various sites and habitats (houses, gardens, markets as well as industrial-like structures) dispersed throughout the city. As part of this project, we here focus on a serologic survey of rodent-borne Toxoplasma, which concerns a sub-total of 46 trapping sites (Figure, ^{Supplementary data}).

A trapping site corresponds either to one or several contiguous gardens (J-CGA, J-CYA, J-DAR, J-KIR1, J-KIR2, J-LMO and J-NOG) (^{Supplementary data}), fallow lands (CRA-1, CRA-2 and CRA-3), administrative buildings (PGP), markets (PEM and GRM-M), industrial food stores (COA, RTO), slaughter house (ABA) or habitation areas (all others) (^{Supplementary data}). All sites lie within the city of Niamey (Figure) (part of a Spot Image, scene reference 506 132 308 121 010 151 32 T, CNES 2008^(c), obtained under licence through the ISIS program, file 553) where they were precisely geo-referenced (e.g., each individual habitation where rodents were captured) in order to be mapped onto a satellite image. However, for the purpose ^{Supplementary data} as well as Figure, they were aggregated for a clearer visualisation at the whole town scale.

Rodents were live-trapped and brought to the lab where they were usually euthanised within one-eight days, except for 45 of them which were autopsied within eight-23 days (data not shown). All procedures were carried out in agreement to current ethical guidelines for animal care. The age was scored according to weight [following Granjon & Duplantier (2009) ] together with sex activity (external testicles plus active seminal vesicles in males; developed mammaes and uterus, presence of embryos and/or embryo scars in females). Intra-cardiac blood was sampled immediately after death and deposited onto LDA22 Guthrie cards (LDA Laboratory, Saint Brieux, France). The blotting papers were dried and stored in a plastic bag at room temperature (RT).

In order to avoid misidentification of rodents due to the possible co-existence of sibling species in West African rodents [reviewed in Granjon & Duplantier (2009) ], special attention was paid to species-specific diagnosis. To do so, specimens were all unambiguously identified (^{Supplementary data}) using morphology-based criteria (genus Cricetomys), karyotyping (Mastomys, Taterillus and Arvicanthis), polymerase chain reaction-restriction fragment length polymorfism (PCR-RFLP) (Mastomys) and/or genotyping (Mastomys and Rattus). All details are provided in Garba (2012).

Serological survey of T. gondii - Dried blood spot samples collected on Guthrie card were tested for the detection of T. gondii antibodies. Seven hundred and sixty six rodents were screened at 1:16, 1:32, 1:320 and 1:640 dilutions using a modified agglutination test (MAT) technique (Desmonts & Remington 1980) adapted for blood sample from Guthrie cards, with a cut-off titre at 1:16. Two 5 mm diameter dried blood spot were punched out of each blotting paper circle and placed into the well of a flat bottomed microtitre plate. The blood was eluted out in 80 µL of phosphate buffered saline, pH 7.2 (bioMérieux). Plates were covered and left to elute overnight at RT and at 300 rpm agitation. Ten microlitres of each eluted sample was used in MAT technique. For serological control, fresh blood from seronegative (not infected by T. gondii) and seropositive (experimentally infected with a control of the presence of cysts into the brain) Swiss mice (Mus musculus, Charles River France, L'Arbresle, France) for T. gondii antibodies were spotted onto a 5 mm diameter circle on Guthrie card and allowed to dry at RT for 24 h, before storage at RT in sealed bags. Antibody titres were determined by the last dilution where agglutination pattern could be read in comparison with the negative and positive controls.

Statistical analysis - Descriptive analyses of the serological data were based on frequencies, percentage for qualitative variables and means, standard deviations for quantitative variables. Relationships between rodent seroprevalence and factors such as sex, species and habitats were investigated through chi-squared test or Fisher's exact test, depending on the expected sample size. For each significant factor, a Cochran-Mantel-Haenszel Chi-Squared test was conducted in order to obtain a p-value adjusted for the other factors. All statistics were performed using the software R v2.10.1 (R Development Core Team 2009).

RESULTS

From the 46 trapping sites sampled for the present study, 766 rodents could be surveyed for Toxoplasma serology: 123 were black rats (Rattus rattus), 61 were house mice (M. musculus), 66 were Nile grass rats (Arvicanthis niloticus), 12 were giant Gambian rats (Cricetomys gambianus), two were slender gerbils (Taterillus gracilis) and 502 belonged to the genus Mastomys (^{Supplementary data}). Among the latter, 287 were investigated using PCR-RFLP designed by Lecompte et al. (2005) and all but two individuals displayed characteristic Mastomys natalensis profiles as defined by Lecompte et al. (2005). Two animals possessed atypical profiles (not shown) and so were fully sequenced for their cytochrome b mitochondrial gene. These DNA sequences allowed to barcode them and to unambiguously identify them as M. natalensis (Dobigny et al. 2008, 2011). In addition, all karyotyped Mastomys (20 of which had not been molecularly characterised) showed a 2N = 32 karyotype typical of M. natalensis (Dobigny et al. 2008). These 307 unambiguously identified M. natalensis represent 61.2% of the whole Mastomys sample available in the present study. Moreover, they originated from all 30 trapping sites were Mastomys individuals were trapped (^{Supplementary data}). No representative of other Mastomys species has ever been found within the city of Niamey even in the framework of wider investigations (n > 650 Mastomys) (K Hima, unpublished observations). We can therefore conclude that all Mastomys that were trapped in the present survey belong to one single species, namely M. natalensis.

Seropositive individuals represent 1.96% of the total rodent samples (15 out of 766) (Tables II, III, ^{Supplementary data}). MAT titres were 1:16 in six, 1:32 in four and 1:640 in five rodents (Table III). The 15 seropositive animals were found in nine different trapping sites (Figure, ^{Supplementary data}) which include CGA, GAW, GNA, GRM, KAR, KAR-1, PEM, J-CYA and J-LMO (Table II, ^{Supplementary data}). They belong to four different species: the native M. natalensis (n = 6 out of 502, 1.2%) and A. niloticus (n = 6 out of 66, 9.1%) and the invasive R. rattus (n = 2 out of 123, 1.6%) and M. musculus (n = 1 out of 61, 1.6%) (^{Supplementary data}). No seropositive individuals were found in C. gambianus and T. gracilis; however, these two species were represented by very low sample sizes (n = 12 and 2, respectively) (^{Supplementary data}).

TABLE II
Rodent captures as well as number of seropositive individuals per species and habitat types

		Rodents (seropositive) n (n)
Species	Total (n)	Industriala	Gardens	Houses	Markets	Seropositive n (%)
Arvicanthis niloticus	66	0 (0)	66 (6)	0 (0)	0 (0)	6 (9.1)
Rattus rattus	122b	82 (0)	3 (0)	27 (2)	10 (0)	2 (1.6)
Mus musculus	61	0 (0)	0 (0)	61 (1)	0 (0)	1 (1.6)
Mastomys natalensis	502	7 (0)	9 (0)	477 (4)	9 (2)	6 (1.2)
Taterillus gracilis	2	0 (0)	2 (0)	0 (0)	0 (0)	0 (0)
Cricetomys gambianus	12	0 (0)	12 (0)	0 (0)	0 (0)	0 (0)
Total	765	89 (0)	92 (6)	564 (7)	19 (2)	15 (1.96)

• a: firms, slaughter house, industrial storage houses and public buildings (Supplementary data); b: one seronegative rat has an ambiguous geographic origin (Supplementary data) and could not be included.

TABLE III
Individual characteristics of all seropositive rodents identified in the present study

Species	Individualb	Sex	Age	Titres	Number of other rodents trapped on the same sitea (n)		Remarks
					Total	Seropositive
Mastomys natalensis (Mn)	NIA 125	M	Ad	1/640	5 Mn	0	-
	NIA 143	M	Ad	1/640	10 Mn	0	-
	NIA 205	F	Ad	1/640	41 Mn	0	-
	NIA 217	M	Ad	1/640	21 Mn	0	-
	NIA 243	F	Juv	1/32	7 Mn + 7 Rr	0	Double capture
	NIA 243b	F	Juv
Mus musculus (Mm)	NIA-GRM-31	M	Ad	1/16	59 Mm + 5 Rr	0	-
Rattus rattus (Rr)	NIA-CGA-13	F	Ad	1/16	1 Mn + 18 Rr	1 Rr	-
	NIA-CGA-5a	F	Ad	1/32	1 Mn + 18 Rr	1 Rr	Double capture with a seronegative juvenile
Arvicanthis niloticus (An)	NIA-CYA-4	F	Ad	1/16	8 Rr	0	-
	NIA-DAR-1	F	Ad	1/640	4 An	0	-
	NIA-LMO-2	F	Ad	1/16	18 An + 2 Cg	3	-
	NIA-LMO-7	F	Ad	1/32	18 An + 2 Cg	3	-
	NIA-LMO-20	F	Juv	1/16	17 An + 2 Cg	2	Triple capture with a third seronegative adult female
	NIA-LMO-21	M	Juv

• a: not necessarily at the same date; b: trapping sites: fallow lands (DAR), garden (CGA, CYA, LMO), market (GRM); Ad: adult; F: female; Juv: juvenile; M: male; NIA: Niamey.

Seropositive individuals included both juvenile and adult animals as well as males and females (Table III). In most instances, they corresponded to one single seropositive specimen found within five-65 specimens from one particular trapping site; only in two exceptions (CGA and J-LMO) did we find several seropositive animals within the same trapping site (Table III, ^{Supplementary data}). Finally, in three instances, seropositive individuals were part of multiple captures (i.e. several rodents trapped together inside the same trap): two juvenile M. natalensis that were both seropositive, one adult R. rattus female trapped with a seronegative juvenile and two juvenile A. niloticus caught with a seronegative female (Table III).

There was no significant relationship between seropositivity and sex of the rodents (p = 0.3). On the contrary, both species and habitat significantly affected seropositivity (p = 0.0017 and p = 0.0001, respectively) with no interaction (p = 0.77). Accordingly, the relationships between species and seropositivity (adjusted for habitat) and habitat and seropositivity (adjusted for species) were both significant by the Mantel Haensel test (p = 0.0001 and p = 0.0001, respectively).

DISCUSSION

The present study, the first one of its kind in Sahel, relies on an important collection of rodent blood samples (n = 766). Represented rodent species are typical Sahelian species that were all already known in the area (Dobigny et al. 2002), with both native (A. niloticus, C. gambianus, M. natalensis and T. gracilis) and invasive (M. musculus and R. rattus) species (Granjon & Duplantier 2009). Although differentiating between rural and urban environments in Niamey may sometimes be tricky since the two types of habitats are often continuous when not fully intermingled (houses closely surrounding or lying within gardens and rice fields, gardens within familial concessions etc), rodent species distribution in regards to biotopes was quite clear: A. niloticus, C. gambianus and T. gracilis inhabit gardens and fallow lands, while M. natalensis, R. rattus and M. musculus are typical commensal animals.

Global T. gondii seroprevalence in rodents from Niamey was low (< 2%), a result that closely matches those found in Gabon during one of the rare other rodent-focused study performed to date in Sub-Saharan Africa (Mercier 2010) (2.3% and 2.7% of 43 commensal and 37 wild rodents, respectively). This parallels previous studies where positive urban rodents are usually rare. For instance, surveys in Brazilian cities showed 4.7% (out of 43 M. musculus and R. rattus), 5% (out of 181 R. rattus) and 0.46% (out of 217 R. rattus, R. norvegicus and M. musculus) of Toxoplasma rodent careers in the cities of Umuarama, Londrina and São Paulo, respectively (Ruffolo 2008, Araujo et al. 2010, Muradian et al. 2012) (see also ^{Supplementary data} for a review about data for rodents in the tropics).

As for other studies, the seroprevalence results may be discussed according to the sensitivity and specificity of the serological test. Seroprevalence in our study was evaluated through a modified-agglutination test which is the most commonly used for defining a possible infection in diverse species of animals, as there is no need for specific secondary antibodies. The cut-off is variable according to species and to studies (1:5-1:25) (Dubey & Frenkel 1998, Dubey 2010). The most commonly considered cut-off is 1:25, but T. gondii has sometimes been isolated from animals with antibody titres below 1:25. That explains why we choose the cut-off of 1:16 that represents the lowest dilution available after elution of dried blood spot. The gold-standard for detection of T. in infected animals and hence to define the true prevalence is a mouse bioassay. This was not possible in the context of Niger. PCR-based method for Toxoplasma DNA detection on tissue samples (brain, muscles) is known to have a lower sensitivity than bioassay and serology (Hill et al. 2006, Truppel et al. 2010).

When considered separately, seroprevalences in Niamey show quite significant variations depending on the species, with low (< 2% in Mastomys, Mus and Rattus) to moderate (> 9% in Arvicanthis) values. This once again fits to what was observed for rodents elsewhere in the World, with species-specific seroprevalence ranging from close to null (e.g., 0.035% of 571 house mice in Panama) (Frenkel et al. 1995) to 100% (e.g., 104 T. swinderianus in Nigeria) (Arene 1986) (^{Supplementary data}). It is also noteworthy that the same rodent species can display extremely different seroprevalence depending on localities or countries. For instance, seroprevalence in R. rattus from Niamey is 1.6% while it reaches 3% (out of 238 black rats) in Micronesia (Wallace 1973a, b), up to 50% (out of 74) in the Philippines (Salibay & Claveria 2005).

These specific as well as geographic variations point toward a complex T. gondii epidemiology that most probably involves several interacting biotic and environmental factors (such as hosts communities structure, individual immunologic characteristics, climatic variables, water, landscape physiognomy and composition, as well as their respective spatio-temporal dynamics), thus making each situation potentially different from one another, even locally (Afonso et al. 2006).

Seropositive rodents were recorded across the year (Table III), encompassing all of the Sahelian seasons [from the warm and dry season (March and April), through the rainy season (June), to the cool and dry season (October and November) ], thus suggesting that Toxoplasma infection may occur throughout the year in Niamey's rodents. However, diachronic monitoring within the same site was not feasible, thus precluding any conclusion about potential seasonal seroprevalence peaks.

Another question about the Toxoplasma sylvatic cycle is vertical transmission from a female rodent to its litter (Owen & Trees 1998, Marshall et al. 2004, Hide et al. 2009). Although our data are limited both in nature (we score antibodies, not proper infection cases) and sample size, we can rely on three instances of multiple hence simultaneous captures to partly address this point (Table III). Indeed, when an adult female is caught with one or several juveniles, one can confidently consider that they are mother and descents; in the same manner, co-captured juveniles have good chances to belong to the same litter (Granjon & Cosson 2008) (and references therein).

First, two seropositive juveniles of multimammate rats were captured together (NIA 243 and NIA 243b) (Table III). Unfortunately, no data about any adult is available here, thus making it impossible to decipher between independent environmental infections - for example at the same place, such as the nest - and vertical transmission. Second, an adult seropositive female of the black rat (NIA-CGA-15a) (Table III) was caught with a seronegative juvenile. Third, a triple capture included a seronegative adult female and two seropositive juveniles of A. niloticus (NIA-LMO-20 and NIA-LMO-21) (Table III). These two latter cases bring poor support (though not refute) to vertical transmission and rather suggest that animals get infected from the environment (soil and water).

Interestingly, the more typical commensal species found in Niamey (M. natalensis, M. musculus and R. rattus) all display low seroprevalences. In particular, only six individuals of the native and widespread species in Niamey, i.e. M. natalensis, were found with detectable Toxoplasma antibodies in spite of a large sample size (n = 501). This species is found within houses in all investigated parts of the city. Importantly, in these urban districts, cats may be numerous since a recent survey in 170 habitations in Niamey revealed that 119 of them (70%) may be associated with the presence of domestic or stray cats (Garba 2012). These cats mainly survive from garbage and wild preys, something that may maximize the risk for them to get infected by ingestion of infected rodents. Low seroprevalence in Mastomys (which is, from far, the dominating species in most habitations, hence the most susceptible to be a major cats' prey) may limit cat predation-mediated infections through commensal rodents, hence in turn decreasing potential transmissions from cats to humans. Another important aspect for public health is the similarly low seroprevalences observed in M. musculus and R. rattus. Indeed, these two invasive species recently established in Niamey (Garba 2012) and it is possible that their populations may potentially extend within the city, potentially partly replacing the native M. natalensis (as this was observed for instance in some parts of Senegal) (Duplantier et al. 1991).

Bovine and ovine meat is traditionally well cooked in Niger. Moreover, no seropositive rodent could be found in our large sample (n = 59 black rats) from the slaughter house (ABA) (^{Supplementary data}). In addition, rodent meat consumption by humans is rather rare in Niger, especially in Niamey and most exclusively concerns young boys that occasionally hunt in gardens. Also, previous studies conducted in Nigeria (Olusi et al. 1994) suggest that rodent meat consumption, even not or poorly cooked, may not play a major role in human contamination. For all these reasons, following previous authors (Develoux et al. 1988, Julvez et al. 1996), we believe that contamination through meat consumption is most probably anecdotal in Niamey.

Low levels of T. gondii prevalence in both human (see above) and rodents (this study) are congruent with Sahelian climatic conditions such as very low hygrometry, soil and air temperatures as well as high ultraviolet irradiations levels which are poorly suitable for oocysts survival and sporulation [Dumas et al. (1991) reviewed in Tenter et al. (2000) ]. This most probably also limits the chance of environmental contaminations. Nevertheless, such extreme and unfavourable conditions may be locally counteracted by human-mediated modifications of the habitat. In particular, the possibly major role of direct waterborne contamination has been receiving increasing support [e.g., reviewed in Jones & Dubey (2010) ]. In the absence of other feasible explanations, water was even speculated as a major source of toxoplasmic infection in pregnant women and children from Northern Niger (Dumas et al. 1991). Interestingly, we found here significantly higher seroprevalence in A. niloticus (9.1%) which, in Niamey, is only found within irrigated gardens (Garba 2012). It was found in six out of the seven gardens that were investigated in the present survey (^{Supplementary data}) and seropositive Nile grass rats were found in three of them (J-CYA, J-DAR and J-LMO) (Figure, ^{Supplementary data}). Unfortunately, we were not able to statistically address this particular issue here, since we could not decipher between Arvicanthis-specific epidemiological properties and environmental (i.e. garden-associated) conditions. If rodent-borne toxoplasmosis was to be more frequent in such habitats/species, as strongly suggested by our data, Toxoplasma human prevalence in Niamey may increase during the coming years, following current extension of irrigated and cultivated surfaces all along the Niger River as well as the Gountou Yena wadi which both cross the city (Djima et al. 2010). Indeed, food habits are clearly switching towards higher consumption of vegetables (e.g., salads, cabbages) that are produced in urban gardens and sold directly in the different markets of town. Sources of watering are the river itself and/or wells where water temperatures should be consistent with oocyst survival (Jones & Dubey 2010). Rodents such as Nile grass rats feed mainly on the cultivated vegetables (Dobigny et al. 2002) (our own observations and many farmers' personal communications). It was previously shown that risk of infection in French cats was higher with warm and moist weather (Afonso et al. 2006). In Niamey, temperatures are always high (the coldest month January is characterised by a normal minimal temperature of 16.6ºC for the 1971-2000 period) (CRA meteorological database) and regular human-mediated irrigation may locally compensate the Sahelian aridity, thus favouring Toxoplasma infection of rodents inhabiting gardens. As such, the connection in Sahelian cities between oocysts, watered vegetables and rodents could be a key element of Toxoplasma circulation that may deserve to be further scrutinised.

To our knowledge, the present study is the first one to focus on T. gondii epidemiology in a Sahelian community of rodents. In spite of a large sample size, seroprevalence was found to be rather low, with a possible exception in A. niloticus that may sign species-specificity and/or a predominant role of water-mediated infection in irrigated gardens. For a clearer view of the whole picture, several aspects need to be investigated. First, a proper study of true infection cases deserves to be conducted to confirm the absence of vertical transmission. Second, other epidemiological agents, such as water, cats, cattle and, of course, human are important to include. Finally, genomic data about of T. gondii that circulate in Africa are very rare (Mercier et al. 2010) and no data exist for Niger. Relevant analyses are thus urgently required to fill this gap since infectivity and morbidity of toxoplasmosis have been related to the protozoan genotype (Ajzenberg et al. 2002, 2009, Boothroyd & Grigg 2002).

Supplementary data

Recapitulation of studies dealing with Toxoplasma seroprevalence in rodents within intertropical regions

Species	Region	Seroprevalence % (n/n)	References
Rodents (not specified)	China	0.9 (9/955)	Lin et al. (1990)
Wild rodents	Gabon	2.7 (1/37)	Mercier (2010)
Bandicota indica	Thailand	2.7 (1/37)	Jittapalapong et al. (2011)
Bandicota savilei	Thailand	0 (0/11)	Jittapalapong et al. (2011)
Cuniculus paca	French Guiana	60.9 (14/23)	Carme et al. (2002)
	French Guiana	60 (22/37)	de Thoisy et al. (2003)
Dasyprocta leporina	French Guiana	23.3 (10/43)	Carme et al. (2002)
	French Guiana	18 (8/45)	de Thoisy et al. (2003)
Hydrochoerus hydrochaeris	Brazil	69.8 (104/149)	Canon-Franco et al. (2003)
	Brazil	75 (49/64)	Yai et al. (2008)
	Brazil	61.5 (16/26)	Truppel et al. (2010)
	French Guiana	6.7 (2/30)	Halos et al. (2007)
Leopoldamys sabanus	Thailand	12.5 (2/16)	Jittapalapong et al. (2011)
Maxomys surifer	Thailand	5.3 (2/38)	Jittapalapong et al. (2011)
Menetes berdmorei	Thailand	7.7 (4/52)	Jittapalapong et al. (2011)
Mus musculus	Brazil	0 (0/19)	Araujo et al. (2010)
	Costa Rica	5 (5/100)	Chinchilla (1978)
	Mexico	3.1 (4/127)	Dubey et al. (2009)
	Panama	0.035 (2/571)	Frenkel et al. (1995)
Myoprocta acouchy	French Guiana	4 (1/26)	de Thoisy et al. (2003)
Niviventer fulvescens	Thailand	0 (0/13)	Jittapalapong et al. (2011)
Rattus spp	Costa Rica	30 (7/23)	Chinchilla (1978)
	Mexico	0.8 (2/249)	Dubey et al. (2009
Rattus exulans	Hawaii	7 (5/85)	Wallace (1973a, b)
	Thailand	1.3 (1/79)	Jittapalapong et al. (2011)
Rattus tanezumi	China	3 (3/101)	Yin et al. (2010)
	Thailand	7.1 (11/156)	Jittapalapong et al. (2011)
Rattus norvegicus	China	3.4 (4/116)	Yin et al. (2010)
	Costa Rica	11.2 (12/107)	Ruiz & Frenkel (1980)
	Egypt	26.7 (16/60)	El Nahal et al. (1982)
	Egypt	34 (34/100)	Rifaat et al. (1971)
	United States of America	12 (2/8)	Burridge et al. (1979)
	Grenada Island	0.8 (2/238)	Dubey et al. (2006)
	Hawaii	1.4 (1/73)	Wallace (1973a, b)
	India	0 (0/186)	Mir et al. (1982)
	Panama	23.3 (52/226)	Frenkel et al. (1995)
	Philippines	60 (50/83)	Salibay & Claveria (2005)
	Thailand	0 (0/34)	Jittapalapong et al. (2011)
Rattus rattus	Africa	8.2 (5/61)	de Roever-Bonnet (1972)
	Brazil	0 (0/24)	Araujo et al. (2010)
	Egypt	42.7 (47/110)	Rifaat et al. (1973)
	Egypt	16.7 (2/12)	El Nahal et al. (1982)
	Florida	13.8 (5/38)	Burridge et al. (1979)
	Gabon	2.3 (1/43)	Mercier (2010)
	Hawaï	8 (36/476)	Wallace (1973a, b)
	Micronesia	3 (7/238)	Wallace (1973a, b)
	Philippines	50 (37/74)	Salibay & Claveria (2005)
Spermophilus variegatus	Mexico	0 (0/69)	Dubey et al. (2009)
Thryonomys swinderianus	Nigeria	100 (104/104)	Arene (1986)

• taxonomic nomenclature follows the last edition of the mammalian systematics reference book (Wilson & Reeder 2005).

Nomenclature, type and Global Positioning System (GPS) coordinates of all 46 trapping sites

Site	Description	GPS		Rodents
		Latitude (N)	Longitude (E)	Species	(n)	Identification	Seropositive (n)
NA	NA	NA		Rattus rattus	1	M	0
ABA	Slaughter house	13.48950	2.12275	R. rattus	59	M, G	0
BAF2	Habitations	13.54401	2.13570	Mastomys natalensis	32	PCR-RFLP (18)	0
BAN	Habitations	13.52161	2.11670	R. rattus	1	M	0
BOU	Habitations	13.53742	2.11331	M. natalensis	46	PCR-RFLP (30), K (4)	0
CGA	Habitations	13.50222	2.11235	M. natalensis	1	PCR-RFLP (1)	0
				R. rattus	19	M, G	2
COA	Habitations	13.53571	2.07399	M. natalensis	2	PCR-RFLP (1)	0
CRA-1	Fallow lands	13.49235	2.09877	Cricetomys gambianus	4	M	0
CRA-2	Fallow lands	13.49655	2.10079	C. gambianus	4	M	0
				Taterillus gracilis	2	K (2)	0
CRA-3	Fallow lands	13.50060	2.10141	Arvicanthis niloticus	4	M	0
CYA	Habitations	13.51204	2.09884	M. natalensis	49	PCR-RFLP (26)	0
				R. rattus	2	M, G	0
DAR	Habitations	13.54624	2.09594	M. natalensis	39	PCR-RFLP (39), K (2)	0
GAM	Habitations	13.49392	2.12501	M. natalensis	18	PCR-RFLP (10)	0
GAM-1	Habitations	13.49792	2.12705	M. natalensis	2	PCR-RFLP (1)	0
GAW	Habitations	13.48970	2.10232	M. natalensis	6	PCR-RFLP (1)	1
GNA	Habitations	13.47908	2.11402	M. natalensis	23	PCR-RFLP (16), K (2)	1
GOU	Habitations	13.51856	2.10883	M. musculus	1	M	0
GRM	Habitations	13.51882	2.11500	M. musculus	60	M, K (5)	1
				R. rattus	5	M, G	0
GRM-M	Market	13.51527	2.11732	R. rattus	3	M, G	0
J-CYA	Industrial store house	13.52029	2.08104	R. rattus	8	M, G	0
	Gardens			A. niloticus	1	M	1
J-DAR	Gardens	13.54714	2.09238	A. niloticus	5	M	1
J-GAM	Gardens	13.48473	2.12775	A. niloticus	11	M, K (2)	0
	Houses within garden			M. natalensis	1	PCR-RFLP (1)	0
J-KIR1	Gardens	13.49397	2.11170	A. niloticus	4	M	0
	Houses within garden			M. natalensis	8	PCR-RFLP (2)	0
J-KIR2	Gardens	13.47573	2.09936	C. gambianus	2	M	0
J-LMO	Gardens	13.50880	2.07810	A. niloticus	19	M, K (2)	4
				C. gambianus	2	M	0
J-NOG	Gardens	13.50558	2.09723	A. niloticus	22	M	0
KAR	Habitations	13.49366	2.09650	M. natalensis	42	PCR-RFLP (6), K (2)	1
KAR-1	Habitations	13.49143	2.08843	M. natalensis	11	K (5)	1
KAR-2	Habitations	13.49316	2.09262	M. natalensis	9	PCR-RFLP (1)	0
KIR	Industrial complex	13.49489	2.10978	R. rattus	16	M, G	0
KIR-1	Habitations	13.48022	2.09984	M. natalensis	5	PCR-RFLP (1)	0
KOT	Habitations	13.58922	2.10928	M. natalensis	10	PCR-RFLP (8)	0
KOU-1	Habitations	13.56106	2.04155	M. natalensis	3	PCR-RFLP (1)	0
LMO	Habitations	13.50696	2.07653	M. natalensis	34	PCR-RFLP (22), K (4)	0
PEM	Market	13.51396	2.10997	M. natalensis	9	PCR-RFLP (3)	2
				R. rattus	7	M, G	0
PGP	Public building	13.52093	2.09161	R. rattus	1	M	0
PKE	Habitations	13.48536	2.10164	M. natalensis	40	PCR-RFLP (23), K (2)	0
REC	Habitations	13.54157	2.08950	M. natalensis	1	PCR-RFLP (1)	0
ROF	Habitations	13.52081	2.15193	M. natalensis	12	PCR-RFLP (9), K (2)	0
ROF-1	Habitations	13.52358	2.14766	M. natalensis	7	PCR-RFLP (2)	0
RTO	Store house	13.49539	2.07916	M. natalensis	5	PCR-RFLP (1)	0
TCH	Habitations	13.58936	2.10137	M. natalensis	16	PCR-RFLP (16)	0
WAD	Habitations	13.51820	2.14351	M. natalensis	10	PCR-RFLP (9), K (2)	0
WAD-1	Coach station	13.51186	2.14032	R. rattus	1	M	0
YAB	Habitations	13.52740	2.08175	M. natalensis	23	PCR-RFLP (10), K (1)	0
YAB-1	Habitations	13.52891	2.08186	M. natalensis	10	PCR-RFLP (1)	0
YAH	Habitations	13.53435	2.08208	M. natalensis	28	PCR-RFLP (17), K (4)	0

• G: genotyping; K: karyotyping; M: morphology; NA: not available (individual from Niamey, but with no precise geographic origin); PCR-RFLP: polymerase chain reaction-restriction fragment length polymorphism.

To D Mazier and the technical team of the Parasitology-Mycology Department (INSERM/UPMC UMR S 945) from the Centre Hospitalier Universitaire Pitié-Salpêtrière (Paris, France), for facilitating our work by welcoming A Mercier in their laboratory, to Isabelle Villena and Dominique Aubert (University of Reims, National Center for Toxoplasma, France), for providing antigen for serological detection.

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• Financial support: CBGP (UMR IRD/INRA/Cirad-Montpellier SupAgro

Publication Dates

• Publication in this collection
  June 2013

History

• Received
  21 Nov 2012
• Accepted
  12 Apr 2013