Background

Hybridization is defined as the interbreeding between individuals or populations that differ by one or more inheritable characters [1, 2]. Such hybridization can have a variety of results, including the promotion of speciation, introgression, vigor and adaptation of hybrids [3] and reverse speciation [4]. As such, hybridization can be considered a significant evolutionary process [5] and this could have positive or negative consequences depending on the taxa [6].

Schistosomiasis is a neglected tropical water-borne parasitic disease of humans and animals, and affects nearly 218 million people in 78 countries with an estimated number of 200,000 deaths per year [7]. About 93% of infected people live in sub-Saharan Africa where widespread poverty and lack of clean water and sanitation contribute to the incidence and spread of the disease [8]. In Africa, the species responsible for this disease were previously grouped into two distinct clades according to their morphology (eggs and adults), the specificity of definitive and intermediate hosts, and their genetics [9]. Thus, one distinguishes (1) the clade Schistosoma mansoni with S. mansoni (a species infecting humans) and S. rodhaini (a species infecting rodents) and (2) the clade S. haematobium with two species infecting humans (S. haematobium and S. guineensis formerly known as S. intercalatum) and six species that mainly infect ruminants and/or rodents (S. bovis, S. curassoni, S. kisumuensis, S. leiperi, S. margrebowiei, S. mattheei) [10, 11]. Schistosomes have a two-host life cycle with an asexual stage developing in a specific freshwater snail host and a sexual stage within the definitive mammalian host from which eggs are discharged into urine or faeces depending on the schistosome species involved. The sexual stage of these dioecious parasites allows interactions between male and female worms within their definitive hosts. Most Schistosoma species are host-specific and geographically separated, which maintains barriers between species and avoids their encounter. However, given the opportunity, heterospecific crosses between species may occur during the sexual stage within the mammalian host. For instance, the clade S. haematobium is frequently involved in hybridization phenomena [11]. Progress in molecular tools has allowed greater exploration of inter-species interactions, particularly between S. haematobium responsible for human urogenital schistosomiasis and its sister species S. bovis [11]. Indeed, S. haematobium and S. bovis are closely related phylogenetically and freshwater snails of the genus Bulinus act as intermediate hosts for both species [12]. This can result in hybridization between the two species, which could influence disease transmission [13]. Several studies have already been conducted on S. haematobium × S. bovis hybrids. They have been identified from samples collected from school-aged children in Niger [14], Senegal [13, 15,16,17,18,19], Benin [20, 21], Mali [22], Côte d'Ivoire [23], Malawi [24] and France [20, 25, 26]. The biological, epidemiological and pathological consequences of this hybridization are still unknown and warrant further investigation due to the potential risk of zoonotic transmission because the infection reservoirs have a significant impact on transmission and therefore on the elimination programme for these worms. Understanding the genetic structure of S. haematobium will lead to a better knowledge of the variation in natural populations and the transmission dynamics of schistosomes between hosts and across geographic origins. Thus, this knowledge of this process may have substantial implications from an epidemiological and evolutionary point of view [27, 28].

In 2005, among the 23 million of Cameroonians, it has been estimated that five million people at risk of schistosomiasis of which two million are infected by one of the three schistosome species (S. haematobium, S. mansoni, S. guineensis) [29, 30], which constitutes a significant human health problem. Efforts are now focused on integrated control strategy including mass drug administration (MDA) with praziquantel primarily aimed at school-aged children, education and social mobilization [31]. Urogenital schistosomiasis caused by S. haematobium is endemic in northern Cameroon, while some foci have been reported in southern Cameroon at Barombi-kotto, Kékem, Kumba, Loum and Marumba [29]. S. bovis is also endemic in this country [32, 33]. Due to the diversity of schistosomes, Cameroon may be a hotspot of schistosome hybrids. Interspecific matings between different species have already been reported between S. haematobium and S. guineensis [34,35,36] and between S. haematobium and S. mansoni [37]. As S. haematobium and S. bovis (a cattle and rodent infecting schistosome) have a wide geographical distribution and several hosts, hybridization involving these two species can be expected to be the most widespread phenomenon in human populations living in Central and West Africa. In domestic cattle, a study based on cercarial shedding and molecular markers reported the presence of hybrids between S. haematobium and S. bovis in Benin [21] but their presence has not been observed in Senegalese and Cameroonian cattle [15, 33]. Our objectives were therefore to verify the presence of hybrids between S. haematobium and S. bovis in Cameroonian humans, to describe how populations of S. haematobium are structured on a large geographical scale, and to examine the impact of these hybrids on the genetic diversity and structure of these populations. Indeed, understanding the extent of hybridization in Cameroonian populations of S. haematobium and its impact on their genetic diversity may shed light on the potential role that hybridization plays in the transmission of urogenital schistosomiasis.

Materials and methods

Studied areas and populations

The study was conducted in 2019 (January–April) in ten geographically distinct populations previously characterized by different infection rates, namely Gazawa Bizili, Guereme, Mokolo and Mourtouwa in the Far North region, Bessoum, Djiporde, Gounougou and Ouroudoukoudje in the North region, Matta Barrage in the West region, and Loum in the Littoral region of the country (Table 1 and Fig. 1). These populations were numbered from 1 to 10 from the south to the north. These localities are well known for their endemicity to S. haematobium [29, 32, 38]. The studied populations consisted of schoolchildren aged 5 to 14 years for whom the parents or legal guardians provided written informed consent on behalf of their children. These children lived in the above localities for at least one year and provided a single urine sample. The child was asked about the possible presence of blood in the urine to confirm the inclusion of these schoolchildren for further investigation. The urine was collected in sterile jars and transferred, in a cooler containing freezing blocks to prevent eggs from hatching, to the nearest health center for further examination. The time between urine collection and examination varied between 1 and 4 h depending on the distance between the site and the laboratory.

Table 1 Description of the sampled localities
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Fig. 1
figure 1

Localities involved in the collection of miracidia

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Parasitological examination and miracidia isolation

From January to April 2019, a total of 225 children aged 5–14 years from the ten locations provide single urine sample. 20–40 ml of urine per child was collected between 10:00 AM and 1:00 PM. Urine samples were transferred to the nearby health centres for parasitological examination. Infection with S. haematobium has been confirmed by the urine filtration technique which allows to identify the presence of schistosome eggs. Each urine sample was vigorously shaken to suspend the eggs and 10 ml were filtered through a 40 µm Nytrel filter before being examined under a microscope to observe the presence of characteristic terminal-spined schistosome eggs. The presence of eggs was recorded, but infection intensities were not determined.

Urine samples from 135 infected children randomly selected were chosen for further analysis. The eggs in the urine samples were placed in fresh water for 10 min to induce the hatching of miracidia. Each larva was then collected using a P10 micropipette (water volume: 5 µl) under a stereomicroscope and preserved on Whatman-FTA® cards (GE Healthcare Life Sciences; Amersham, UK). Each card received 20–30 miracidia isolated from each other and was stored at room temperature (20–30 °C). FTA Card were the transferred to the University of Perpignan in France for molecular analysis that started in January 2020.

Molecular biology

DNA from individual miracidia was extracted using the protocol described by Beltran et al. [39] and genotyped using three distinct genetic markers: mitochondria Cox1 gene using Rapid Diagnostic (RD)-PCR method [40], nuclear internal transcribed spacer 2 (ITS 2) gene using PCR-Restriction Fragment Length Polymorphism (RFLP) method [40] and a panel of 14 microsatellite markers [41]. The methods are detailed below.

The percentage of hybrids between S. bovis and S. haematobium was assessed using a classical method based on the discordance in species identification between mitochondrial (Cox1) and nuclear (ITS2) markers. Schistosome species identification using Cox1 was evaluated using a rapid detection PCR method described by Angora et al. [23]. This PCR includes a non-specific forward primer and three specific reverse primers targeting S. mansoni, S. haematobium or S. bovis. After PCR and agarose gel electrophoresis, the amplicon size indicates the schistosome species [23]. Species identification using the nuclear gene (ITS2) is more complex because this nuclear marker can be homozygous or heterozygous. The method used was a classical PCR using non-specific primers followed by enzyme restriction cutting on the mutation points differentiating S. bovis from S. haematobium. The ITS2 fragment was first amplified by either a previously published primers (Forward: 5′-TCCTCCGCTTATTGATATGC-3′ and reverse: 5′-GGAAGTAAAAGT-CGTAACAAG-3′), which generated a 981 bp fragment [40] or newly defined primer (Forward: 5′-GGCTGCAGCGTTAACCATTA-3′ and reverse: 5′-ACACACACCATCGGTACAAA-3′) which generated a shorter 505 bp fragment. We used these last primer pair on 59% of the samples because we failed to amplify a long 981 bp fragment certainly due to DNA degradation. Both amplified fragments, the shorter and the longer include mutations differentiating S. bovis from S. haematobium. In a second step, the amplified fragments were digested with the MboI enzyme (New England Biolabs, Evry, France), which produced (1) for the 981 bp amplicon fragments of 36, 85, 100, 130, 174 and 280 bp for S. haematobium, and fragments of 36, 83, 130, 167, 174 and 380 bp for S. bovis [40] (2) for the 505 bp amplicon fragments of 44, 82 and 379, a for S. haematobium, and fragments of 44, 82, 98, and 281 bp for S. bovis (See Additional file 1). The combination of Cox1 and ITS2 markers resulted in six different possible genotypes (Cox1_ITS/ITS): two genotypes are considered pure parasites (Sb_Sb/Sb, Sh_Sh/Sh) and four genotypes are considered hybrids (Sh_Sb/Sb, Sb_Sh/Sh, Sh_Sh/Sb, Sb_Sb/Sh). The percentage of hybrids in the different populations was tested using the χ2 test under the null hypothesis of equal distribution.

Each miracidium was genotyped using a set of microsatellite markers previously developed for S. haematobium [41] as these markers have recently been found to cross-amplify with S. bovis [33]. These markers are grouped in two multiplexes of 9 microsatellites ranging from 183 and 366 bp: panel 1 (C102, Sh1, Sh14, C131, Sh6, Sh9, Sh13 and Sh7) and panel 2 (Sh2, Sh5, Sh13, Sh4, Sh10, Sh12, Sh8, Sh11 and Sh15). Of the 18 microsatellites tested, 14 successfully amplified the parasite samples and were therefore used in the present study. The remaining four markers (C131, Sh4, Sh8 and Sh15) were successful on less than 20% of the specimens and were eliminated from our dataset. Microsatellite amplifications were performed using the Qiagen® Multiplex PCR kit (Qiagen, Hilden, Germany). Forward primers were fluorescenced using 6-FAM, VIC, NED and PET dyes (Applied Biosystems, Foster City, USA) according to Webster et al. [41]. The PCRs were performed according to the manufacturer’s standard microsatellite amplification protocol, with the exception of the final volume of 10 μl which includes 2.5 μl of DNA template. Thermal cycling was performed with an initial 15-min hot activation at 95 °C, followed by 30 cycles of 94 °C for 30 s, 56 °C for 90 s and 72 °C for 60 s, with a final extension at 60 °C for 30 min. This amplification was performed using a TECNE TC-Plus thermal cycler (Cole-Palmer, Stone, UK). Microsatellite reactions were sent to a subcontractor (Genoscreen company, Lille, France) for genotype determination. Peak calling and genotype determination were performed using GeneMarker software (https://softgenetics.com/). Automatic allele size determination was performed using the Fragment Animal Analysis option of Genemarker software with the GS500 size standard. Each allele determination was double checked by visual inspection and the microsatellite matrix was exported as a data spreadsheet.

Population genetic analyses from microsatellites

Linkage disequilibria and deviations from Hardy–Weinberg’s expectations were tested using exact tests (1,200 permutations) as implemented in the FSTAT software, version 2.9.3.2 [42]. The significance level has been adjusted for multiple tests using the standard Bonferroni corrections [43]. The genetic diversity of the miracidia of each population was assessed by calculating the expected heterozygosity (He) and the allelic richness (Ar) using the FSTAT software, version.2.9.3.2 [43]. These population-to-population parameters were compared using Friedman’s pairwise rank tests, followed by Nemeyi’s multiple comparison test implemented in the Rstudio PCMPplus package. The link between the genetic diversity indices (He or Ar) and the percentage of hybrids was assessed using linear regression method of SPSS 18.0 (SPSS Inc., Chicago, USA). In addition, after identifying the hybrids, we calculated the number of private alleles they carried in their respective populations.

Genetic differentiation between localities was assessed using pairwise FST values according to Weir and Cockerham [44]. We calculated these values and their associated significance using global tests implemented in the FSTAT software, version 2.9.3.2 [42] with a significance threshold adjusted for multiple tests according to Bonferroni’s standard corrections [42]. In addition, at the individual level, we combined Euclidian geographic distances (calculated from geographic coordinates) and genetic distances in a simple Mantel test using Genetic differentiation between sites was assessed using pairwise FST values according to Weir and Cockerham [44]. We calculated these values and their associated significance using global tests implemented in the FSTAT software [42] with significance threshold adjusted for several tests according to Bonferroni’s standard corrections [42]. In addition, at the individual level, we combined Euclidean geographic distances (calculated from geographic coordinates) and genetic distances in a simple Mantel test using GenAlEx 6.51b2 [45]. Finally, we determined the highest level of genetic structure for all individuals using the Bayesian clustering approach implemented in the STRUCTURE software, version 2.3 [46]. The run-in period for each trial was set to 50,000, followed by 500,000 MCMC iterations. We performed 10 independent runs for each K value from 1 to 12. We estimated the most likely number of genetic clusters (K) using the method implemented in the STRUCTURE HARVESTER, version 0.6.9 [47, 48]. Finally, we determined the uppermost level of genetic structure of all individuals using the Bayesian clustering approach implemented in the STRUCTURE software, version 2.3 [46]. The run-in period for each trial was set to 50,000, followed by 500,000 MCMC iterations. We performed 10 independent runs for each K value from 1 to 12. We estimated the most likely number of genetic clusters (K) using the method implemented in the STRUCTURE HARVESTER, version 0.6.9 [47, 48].

Results

Hybrid identification

A total of 1,327 miracidia coming from eggs collected from 55 children were successfully genotyped (Table 2). Most of them (88.7%) were identified as pure genotypes of S. haematobium (Sh_Sh/Sh) while the others (11.3%) were hybrids (7.0% with Sh_Sh/Sb, 3.7% with Sb_Sb/Sh and 0.4% with Sb_Sh/Sb). No miracidia were identified as pure genotypes of S. bovis. The great majority of Cox1 and ITS2 alleles were from S. haematobium (95.8% and 96.2%, respectively). A significant variation (\({\chi }^{2}\) = 22.27, df = 9, P < 0.01) in the relative number of these hybrids has been observed according to the locality, ranging from 3.6% for Mokolo to 21.2% for Matta Barrage.

Table 2 Number of hybrids and pure schistosome genotypes recovered in each sampled locality
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Genetic diversity

Although no evidence of link disequilibrium was detected (P-value threshold after Bonferonni’s standard correction: P = 0.0005), we noted deviations from Hardy–Weinberg’s expectations among several pairs of loci/populations (P < 0.0004, significance threshold adjusted with the Bonferroni procedure for 140 tests) (Additional file 2).

Mean allelic richness ranged from 5.55 to 7.73 for populations from Loum and Matta Barrage, respectively (Table 3). A significant difference was observed according to the different populations (χ2 = 47.20, df = 9, P < 0.001). Post-hoc Nemeyi test identified significant differences (1) between population 1 and populations 2, 4, 6 and 9, (2) between population 7 and populations 2 and 6, and (3) between population 8 and populations 4 and 6. Mean heterozygosity ranged from 53.7% to 59% for Loum and Matta Barrage, respectively (Table 3). No significant differences in heterozygosity were observed among the different populations. Interestingly, allelic richness (r = 0.71, df = 9, P < 0.05) and heterozygosity (r = 0.87, df = 9, P < 0.05) were positively related to the percentage of hybrids recovered in the 10 populations sampled (Fig. 2). Except in Guereme, the identified hybrids carried private alleles (between 1 and 7) in their respective populations (Additional file 2).

Table 3 Mean allelic richness (Ar) and heterozygosity (He) recorded for the ten miracidia populations coming from ten endemic localities in Cameroon
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Fig. 2
figure 2

Relationship between heterozygosity (A) or allelic richness (B) and the percentage of Schistosoma haematobium × S. bovis hybrids in Cameroon. The number associated to the dots refers to the population number (see Table 1)

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Population structure of Schistosoma haematobium

After Bonferroni’s adjustment, pairwise genetic differentiation estimates (FST) were all significant (P < 0.001) and ranged from 0.006 (between Gounougou and Djiporde) to 0.097 (between Loum and Mokolo) with a mean FST value of 0.039 (Table 4). The Mantel test between genetic (FST) and geographic distance matrices revealed a significant association, suggesting an Isolation by Distance (IBD) model with P < 0.001 (Fig. 3). STRUCTURE and STRUCTURE HARVESTER results inferred the highest ΔK value for K = 3 (Additional file 3). However, the ΔK value was very low, suggesting little convergence between the 10 independent runs.

Table 4 Pairwise genetic differentiation estimates (FST: above the diagonal) and geographic distances (Km: under the diagonal) between the 10 sampled populations. All FST values are significant (P < 0.001)
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Fig. 3
figure 3

Relationship between geographic distances (measured as Euclidian distances between sites) and genetic distance (estimated with FST values between sites)

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Discussion

Basic analysis on our microsatellite dataset showed deviation from Hardy–Weinberg’s expectations among several pairs of loci/populations. However, it is difficult to interpret these deviations from Hardy–Weinberg’s expectations, as the populations analyzed include parasites collected from several hosts and not a panmictic parasite populations. Thus, this absence of Hardy Weinberg’s equilibrium and especially the excess of homozygote could be due to a Wahlund effect resulting from a sampling in different hosts.

Few populations genetic studies have been undertaken on S. haematobium compared to S. mansoni (see [49] for a review). According to these studies, S. haematobium populations are generally less genetically structured than those of S. mansoni [49, 50]. To document the divergence between S. haematobium populations at different Cameroonian localities, genetic differentiation (FST) was calculated for all possible pairs. The measurement of FST values provides information on the population substructure and is useful for examining the overall genetic differentiation/divergence between populations. FST values below 0.05 indicate low genetic differentiation, while values between 0.05 and 0.15, 0.15 to 0.25, and above 0.25 indicate moderate, high, and very high genetic differentiation, respectively [51]. In the present study, the paired FST values between populations were low to moderate. The most differentiated populations were between Loum and Mokolo (FST = 0.097), while the least differentiated were between Djiporde and Gounougou (FST = 0.006). These FST values were consistent with previous results on S. haematobium showing either a lower FST value for shorter distances between sites (FST = 0.4% between 8 km separated sites [52]) or higher FST values for higher distances between countries (FST = 17.3% between Cameroon, Kenya, Mali, Niger and Tanzania [49]). As a result, our findings reveal a significant pattern of IBD. By comparing parasites from separate countries at the continental level, IBD was previously observed using a microsatellite dataset [49] but was not confirmed using SNP [53]. The overall genetic differentiation inferred either by a principal component analysis or by the Bayesian approach showed a partial structure. In the Bayesian method the ΔK value was very low, suggesting little convergence between the runs. This echoes the fact that the Bayesian method implemented in the STRUCTURE software is sensitive to IBD patterns and may discern multiple clusters where there is only a single large area with IBD [54]. Moreover, the ΔK method often fails to find the best K if K = 1. Thus, the Bayesian clustering method seems to indicate a weak genetic structure. Southern populations (Loum and Matta Barrage) were clearly separated from other localities, but genetic differentiation between northern localities was limited, certainly due to the geographic proximity between these sites. There is no link between the snail host species involved in local transmission (Table 1) and genetic structure.

Our study enabled to identify S. haematobium × S. bovis hybrids in the ten studied sites. The presence of S. haematobium × S. bovis hybrids has already been reported in humans in several West African countries including Benin, Côte d’Ivoire, Niger and Senegal [11, 13, 23]. These hybrids were also involved in the recent schistosomiasis outbreak in Corsica both during the first emergence in 2013 [25] and in recurrent infections in summers 2015, 2016, 2017 and 2018 [55,56,57]. In this case, the emerging parasite has been shown to originate from a West African country [25]. Using the same molecular discrimination method (i.e., identification of schistosome species based on Cox1 and ITS2), previous studies have revealed various frequencies of these hybrids. In Senegal and Benin, 21–22.6% (n = 823) and 29.8% (n = 47) of parasites, respectively, were classified as hybrids [15, 21]. At only 11.3%, the mean frequency of hybrids in Cameroon appears low compared to those in other countries. In Benin, the percentage of these hybrids was noted in a single locality [21], while in Senegal it varied between sites from 16.3% (Barkedji) to 62.5% (Sinthiou Malem) [15, 58]. As the percentages ranged from 2.7 to 21.2% in the present study, the distribution of hybrids is therefore uneven among the populations sampled in Cameroon. Most important is the fact that these percentages of hybrids are related to the genetic diversity of the parasite (measured by allelic richness and heterozygous), highlighting that hybridization is a major biological process that shapes the genetic diversity of S. haematobium. During the introgression process, the addition of new alleles of a given species (S. bovis) is expected to increase the genetic diversity of the introgressed species (S. haematobium). This increase in genetic diversity is also supported by the fact that S. bovis is a genetically different parasite than S. haematobium [33, 59]. If this result is expected, the ecological consequences are important because this indicates that genetic introgression occurs in Cameroon and is certainly a current and dynamic process. Recently, two genome-wide studies have suggested that hybridization between S. bovis and S. haematobium would certainly be an ancient event [53, 60]. However, this does not mean that the genetic mixture between S. haematobium and S. bovis would not always be ongoing. This latter hypothesis does not seem to be supported by the fact that we did not find hybrids in Cameroonian cows [33]. While the S. haematobium genome is currently introgressed by S. bovis genes, human-caused parasite populations must be regularly maintained by S. bovis alleles.

Three non-exclusive hypotheses can be proposed to explain these apparently discordant results. The first hypothesis is that S. haematobium × S. bovis hybrids would exist in Cameroonian cows, but we have not been able to identify them. Indeed, in our study on these animals, we did not select a given transmission site characterized by a close proximity between humans and animals because these cows were randomly selected in slaughterhouses [33]. In addition, our results reveal a non-homogeneous spatial distribution of hybrids in Cameroonian humans. This first hypothesis is also supported by the fact that in such a context of human/animal proximity, S. haematobium × S. bovis hybrids have been identified in both humans and cows in Benin [21]. In contrast, no hybrids were found in cows in Senegal [15, 16] and no trace of recent hybridization was noted in the genome of S. haematobium from Niger and Zanzibar [60]. The second hypothesis is that these hybrids would exist in a host animal which is not the cow. S. bovis infects a variety of animals such goats, sheep or rodents [61]. Until the recent discovery in Benin, no hybrids had yet been found in cows and rodents were proposed as hosts for the encounter between S. haematobium and S. bovis [13].

Recently, these hybrids have been found in rodents in both Senegal and Corsica with a very variable prevalence and intensity [17, 62]. The existence of an asymmetric infection process could be the third hypothesis: pure genotypes of S. bovis from animal origin would be able to infect humans as does S. haematobium, but their hybrids could not develop in animals.

Increasing genetic diversity through introgression of interspecific genes can have important implications in terms of disease control and outcome. First, there is an expectation that there will be more genetic variants and that there will be more potential resistance to treatment. Second, genetic variation may also be important in the intensity of the parasite and the subsequent outcome of the disease. Using non-informative genetic markers (RAPD), no link was observed between heterozygosity and the severity of infection, but a positive link between genetic clusters, bladder or kidney pathology, and the intensity of infection was observed [63]. Only one study showed a clear association between allelic variation, expressed as the presence of a specific allele, infection intensity and associated bladder morbidity [64]. It seems evident that more studies are needed to infer the potential consequences of genetic diversity of parasites on disease outcomes [50].

One important limitation of the study is the use of a rapid identification method such RD-PCR or PCR–RFLP which cannot identify single species. The PCR–RFLP does not differentiate S. bovis from S. guineensis or S. curassoni. S. guineensis is known to be historically present in the equatorial zone of Cameroon (areas of the sites 1 and 2 of the present study) and S. guineensis × S. haematobium hybrids have already been identified in Cameroon [65]. Consequently, in sites 1 and 2 we may have identified some S. guineensis × S. haematobium hybrids but defined as S. haematobium × S. bovis hybrids. By removing the sites 1 and 2 from the analyses, with only 8 points in the regression, the association between hybrid percentage and heterozygosity remains significant (P < 0.05) but not between hybrid percentage and allelic richness (P > 0.05). Regarding S. curassoni its precise distribution is unknown but this parasite is present in west Africa and S. haematobium × S. curassoni hybrids has been evidenced in Senegal [15]. If the PCR–RFLP cannot distinguish S. bovis from S. curassoni, the RD-PCR produces double-band profile for S. curassoni and single-band profile for S. bovis [66]. On the 1327 miracidia we did not observe RD-PCR double-band profile and thus we hypothesis that we did not have S. curassoni in our sampling. The only way to distinguish between all these pathogens is Sanger sequencing which remains an expensive method. The main conclusion of the manuscript does not change. The genetic introgression via hybridization with a distinct S. haematobium species whether S. guineensis or S. bovis (or a mix) increases the genetic diversity of S. haematobium.

Conclusions

Hybrids between S. haematobium and S. bovis were found in 11.3% of miracidia that hatched from eggs present in the urine of schoolchildren in 10 Cameroonian localities. The percentages of these hybrids are related to the genetic diversity of the parasite, which highlights the fact that hybridization is a major biological process that shapes the genetic diversity of S. haematobium and more generally that of parasite species.