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Infection susceptibility and vector competence of Rhodnius robustus Larrousse, 1927 and R. pictipes Stal, 1872 (Hemiptera, Reduviidae, Triatominae) for strains of Trypanosoma cruzi (Chagas, 1909) (Kinetoplastida, Trypanosomatidae) I, II and IV
Parasites & Vectors volume 15, Article number: 239 (2022)
Rhodnius robustus and Rhodnius pictipes are vectors of Trypanosoma cruzi, the etiologic agent of Chagas disease (CD), that are found in the Brazilian Amazon region. Susceptibility to infection and vector competence depend on the parasite-vector relationship. Our objective was to evaluate the interaction between T. cruzi and these two triatomine vectors in pure and mixed experimental infections of T. cruzi strains from the same or different geographic regions.
Fifth-instar nymphs of R. robustus and R. pictipes were fed on mice infected with four T. cruzi strains, namely genotypes TcIAM, TcIMG, TcIIPR, and TcIVAM, respectively, from the Brazilian states of Amazonas, Minas Gerais and Paraná. Over a period of 120 days, excreta were examined every 20 days to assess vector competence, and intestinal contents (IC) were examined every 30 days to determine susceptibility to infection.
The highest positive rate in the fresh examination (%+FE, 30.0%), the highest number of parasitic forms (PF, n = 1969) and the highest metacyclogenesis rate (%MC, 53.8%) in the excreta were recorded for R. robustus/TcIVAM. Examination of the IC of R. pictipes revealed a higher number of PF in infections with TcIAM (22,680 PF) and TcIIPR (19,845 PF) alone or in association (17,145 PF), as well as a %+FE of 75.0% with TcII, in comparison with the other genotypes. The highest %MC (100%) was recorded for the mixed infections of TcIAM with TcIIPR or TcIVAM in the IC of R. pictipes.
Overall, both species were found to be susceptible to the T. cruzi strains studied. Rhodnius robustus showed vector competence for genotypes TcIVAM and TcIAM+TcIVAM and R. pictipes for TcIAM+TcIVAM and TcIAM+TcIIPR; there was elimination of infective forms as early as at 20 days. Our results suggest that both the genetics of the parasite and its geographic origin influence the susceptibility to infection and vector competence, alone or in association.
Trypanosoma cruzi is a hemoflagellate protozoan that is the etiologic agent of Chagas disease (CD), also known as American trypanosomiasis . Triatomine insects (Hemiptera, Reduviidae, Triatominae) serve as vectors, while the vertebrate hosts can be wild and domestic mammals, as well as humans . While CD is endemic in Latin America, globalization and human migrations have been major factors in its spread to countries considered to be non-endemic where it has become an important disease. According to the WHO, 6–7 million people are infected with CD worldwide , and it is estimated that 62.4% of these reside in the countries belonging to the Southern Cone of South America (Argentina, Brazil, Chile, Paraguay and Uruguay) .
This parasite has a wide genetic diversity, and its strains are classified into six discrete typing units (DTUs), TcI to TcVI [5, 6]. Trypanosoma cruzi I (TcI) is the DTU most frequently isolated from the wild, and its presence has been reported in different triatomine species of the genus Rhodnius Stål, 1859. This strain typically causes heart disease in northern South America . TcII has been isolated from triatomines of the genus Panstrongylus Berg, 1879 and wild animals (Didelphis sp. and Euphractus sp.). This strain generally causes cardiac and digestive CD in infected persons in southern South America (South Cone countries) and occurs more frequently in the domestic transmission cycle . TcIII and TcIV are less frequently isolated from the wild and are associated with outbreaks of oral CD in the Amazon, with the latter associated with heart disease in northern South America. TcIV has only been isolated from the species Rhodnius robustus Larrousse, 1927 and Rhodnius brethesi Matta, 1919. TcV and TcVI are considered to be hybrid strains that occur in the domestic transmission cycle. Recently, TcBat, the seventh DTU, was identified. This genetic lineage is associated with bats, based on its detection in both insect and fruit-eating bats in China, but its presence in humans has already been demonstrated by molecular techniques. Phylogenetic analysis, based on PCR amplification of a multicopy amplicon targeting members of the trans-sialidase family and large-scale sequencing, has confirmed that TcBat is indeed a DTU distinct from the others and suggests a scenario in which it is more closely related to TcIII than to TcI [7,8,9,10]. As yet, there are few studies on TcBat and its possible clinical manifestations in humans .
The vectors of CD are arthropods belonging to the Triatominae subfamily, which are distributed in five tribes and 18 genera, encompassing around 157 species (154 living species and three fossils) [12,13,14,15,16]. The genera Panstrongylus and Triatoma Laporte, 1832, as well as the genus Rhodnius, play an important role in the epidemiology of CD. The genus Rhodnius comprises 21 species [16,17,18], including R. robustus and R. pictipes Stal, 1872, which inhabit different species of wild and peri-urban palm trees. The winged adults can invade human dwellings and their dependencies without colonizing them [19, 20]. In the Brazilian state of Amazonas, palm tree populations act as sources of adult adventitious bugs of R. robustus sensu lato, R. pictipes and R. brethesi (these species have high rates of infection by trypanosomatids), leading to the contamination of food-processing equipment and, subsequently, the emergence of acute cases of oral CD, or to the attack of forest workers by these bugs, leading to isolated cases of vector transmission [19, 21,22,23].
In studies on the interaction of different strains of T. cruzi with the main vector species, variations in both protozoan population density and insect infection rates have been reported [2, 24,25,26]. The mean positivity rates among different triatomine species ranged from 9.8% in Triatoma dimidiata Latreille, 1811 to 91.4% in Triatoma pseudomaculata Corrêa & Espínola, 1964, with an overall mean positivity rate of 67.3% .
Although the complex interaction between T. cruzi and its vector for transmissibility is not yet fully understood, it is known that this interaction can be influenced by the biological, biochemical and genetic characteristics of both the vector and the parasite, combined with the fact there are sympatric species that are better adapted to the environment in which they are inserted [26,27,28,29]. In addition, the hematophagous habits of the vectors contribute to the selection of populations of T. cruzi, in that some genetic lineages can be eliminated while in others an increase in the population can occur, even when they are concomitant in the vector . In this context, the objective of the present study was to evaluate the susceptibility to infection and vector competence of triatomine species from the Amazon region, both with strains from the same region and with those from other geographic areas of Brazil.
The use, maintenance and care of the mice in the present study followed the guidelines of the Conselho Nacional de Controle de Experimentação Animal (CONCEA), and the project was approved by the Comissão de Ética no Uso de Animais of Universidade Estadual de Maringá (CEUA/UEM) (Registration no. 9659251017). The use of T. cruzi strains obtained from humans was approved by the Ethics Committees of the Fundação de Medicina Tropical Doutor Heitor Vieira Dourado (Registration no. 360/07) and of UEM (Registration no. 100/04 e 375/07).
Triatomines and their maintenance
The colonies of R. robustus species used in this study are derived from Loreto, Peru , and those of R. pictipes species were originally from Serra Norte, Pará State, Brazil . Rhodnius robustus and R. pictipes were kindly donated by the Laboratório Nacional e Internacional de Referência em Taxonomia de Triatomíneos, at Instituto Oswaldo Cruz/Fiocruz. The insects were kept under controlled conditions of temperature (appox. 26 °C), relative humidity (approx. 60%) and light (light/dark cycle: 12/12 h), and regularly fed on Swiss mice previously anesthetized in the Parasitology Sector of the Department of Sciences Health Basics of Universidade Estadual de Maringá (UEM).
T. cruzi strains
Four T. cruzi strains belonging to three different DTUs (TcI, TcII and TcIV) and originating from three Brazilian states (Amazonas, Minas Gerais and Paraná) were used. Two strains belong to the DTU TcI: PR150, isolated in 1990 from a patient in the chronic phase of the disease in Paraná, but originally acquired in Minas Gerais (TcIMG) , and AM33, isolated from R. pictipes captured in Manaus, Amazonas (TcIAM) in 2007 . The other strains used include one belonging to DTU TcII, PR1256, which was isolated from a chronic case in Paraná in 1992 (TcIIPR) , and one belonging to DTU TcIV, AM14, which was isolated from an acute case acquired orally in Coari, Amazonas in 2007 (TcIVAM) .
Inoculation of animals
Male Swiss Mus musculus mice aged 21–28 days and weighing between 18 and 22 g were used. The mice were housed in polypropylene cages maintained under a 12 h/12-h light/dark cycle; food and water were available ad libitum. The inoculum consisted 2 × 106 culture-derived metacyclic trypomastigotes (CMT) from each of the four strains used in the study, in 1.0 ml of liver infusion tryptose (LIT) culture medium . The mice were infected through intraperitoneal injection of the inoculum. In mixed infections, two strains were used in each injection, with equal amounts of each strain.
Infection of triatomines
Triatomine species from the Amazon region (R. robustus and R. pictipes) were infected with strains of T. cruzi from the same region and from other geographic areas (Minas Gerais and Paraná States). In total, 180 fifth-instar nymphs of each species were used. As a negative control in the PCR analysis, 20 uninfected nymphs of each species were used.
For each triatomine species, the fifth-instar nymphs were divided into groups of 20 specimens each, for a total of nine experimental groups: (i) four groups fed on mice inoculated with a single strain of T. cruzi (pure infections); (ii) five groups fed on mice inoculated with two strains at the same time (mixed infections); (iii) and one group was uninfected (control group: fed on healthy mice). The groups (G) were arranged as follows: G1 (TcIAM), G2 (TcIMG), G3 (TcIIPR), G4 (TcIVAM), G5 (TcIAM+TcIVAM), G6 (TcIAM+TcIIPR), G7 (TcIMG+TcIIPR), G8 (TcIMG+TcIVAM) and G9 (TcIIPR + TcIVAM), for both triatomine species (Fig. 1).
Excreta were examined every 20 days for up to 100 days to assess vector competence, and intestinal content (IC) was examined every 30 days for 120 days to determine susceptibility to infection.
Insects from groups G1 to G9 were fed on mice previously inoculated via the intraperitoneal route, on the day of maximum parasitemia peak. In pure infections, the maximum peak of parasitemia occurs on the seventh day post-infection (dpi) for strains AM33 (TcIAM) and AM14 (TcIVAM), and on the 13th dpi for strains PR150 (TcIMG) and PR1256 (TcIIPR). In mixed infections (TcIAM+TcIIPR, TcIAM+TcIVAM, TcIMG+TcIIPR, TcIMG+TcIVAM and TcIIPR+TcIVAM), the insects were fed both on the seventh and 13th dpi, according to the parasitemia curve profiles of each strain, which our group has previously described [33, 37, 38]. At the peak of parasitemia, the mice had approximately 1400 blood trypomastigotes (BT) per 0.1 ml of blood [37, 39], both for the pure infections with one strain (TcIAM, TcIMG, TcIIPR or TcIVAM) and for the mixed infections containing two strains (TcIAM+TcIIPR, TcIAM+TcIVAM, TcIMG+TcIIPR, TcIMG+TcIVAM and TcII+TcIVAM).
The triatomines were kept under controlled conditions of temperature (28 ± 1 °C), relative humidity (60 ± 5%) and photoregimen (12/12-h light/dark), in a Biochemical Oxygen Demand (BOD) in the Parasitology Sector of the Department of Basic Health Sciences.
Determination of blood volume and number of forms ingested
The nymphs were weighed individually in a group of 20 insects for each experimental group, with a semi-analytical scale (model BK 300; Gehaka, São Paulo, Brazil) before and after the blood meal. Nymphs with a weight gain ≥ 1.0 mg after feeding were considered to be fed. To estimate both the blood volume and the number of ingested parasites, a 1.0 mg weight gain was considered to be equivalent to 1.0 µl of ingested blood .
The mean number of blood forms ingested was determined from the mean blood volume ingested per group × 1400 BT/0.1 ml of blood .
Analysis of excreta to determine vector competence
Triatomines were fed every 20 days with blood from uninfected mice sedated with a solution of ketamine (100 mg/kg) + xylazine (5–10 mg/kg) (1:2), according to CONCEA guidelines, and monitored for a period of 120 days. During or after the blood meal, the excreta (feces and urine) eliminated spontaneously were collected and added to 100 μl of phosphate-buffered saline (PBS) at 0.15 M (pH 7.2). A 5-μl aliquot from the pool of excreta was used to perform the fresh examination (FE), in duplicate, under an optical microscope, at a magnification of 400× .
A 10-μl aliquot of the pool of excreta was used to prepare smears stained with Giemsa for the differential count (DC), in duplicate, to determine the number of metacyclic trypomastigote (MT), epimastigote (EP) and spheromatigote (SF) forms per group, reading the entire smear with an immersion objective (magnification: 1000×) [40, 41]. The metacyclogenesis rate (%MT; the proportion of metacyclic forms in relation to the total number of parasitic forms) was computed considering only the EP and MT forms and calculated for each experimental group [40, 41].
Analysis of IC to determine susceptibility to infection
Every 30 days, for a period of 120 days, the intestines of five specimens from each group were removed and macerated with 100 μl of PBS at 0.15 M, following which a 5-μl aliquot of the macerate was freshly examined (FE)  and a 10-μl aliquot were used to make a smear stained with Giemsa, in duplicate. The parameters to be observed were the same as described above for excreta. The samples were added to 500 µl of 70% alcohol, which were stored at −20 ºC until DNA extraction.
PCR analysis of T. cruzi kinetoplast DNA
Kinetoplast DNA–PCR (kDNA-PCR) was used to verify the infection of negative insects in the FE. For this, the DNA of T. cruzi was extracted from the pool of excreta and IC of the insects using the conventional method of phenol/chloroform described by Macedo et al. . Primers 121 (5′-AAATAATGTACGGG[T/G]GAGATGCATGA-3′) and 122 (5′-GGTTCGATTGGGGTTGGTGTAATATA-3′) were used to amplify (35 cycles; Techne™ TC-512 thermocycler; Thermo Fisher Scientific, Waltham, MA, USA) a 330-bp fragment of the T. cruzi kDNA). PCR products were visualized on a 4.5% polyacrylamide gel by silver staining, as described by Miyamoto et al. . The 100-bp DNA molecular weight marker from Invitrogen™ (Thermo Fisher Scientific) was used to confirm the correct size of the analyzed fragment.
Restriction fragment length polymorphism of the cytochrome oxidase subunit II gene
Amplification of the cytochrome oxidase subunit II (COXII) gene by PCR followed by restriction fragment length polymorphism (RFLP) analysis with the restriction enzyme AluI was used to differentiate DTUs I to VI. The amplification of the COXII gene was performed according to Abolis et al.  and Sá et al. , using primers Tcmit-10 (5′-CCATATATTGTTGCATTATT-3′) and Tcmit-21 (5′-TTGTAATAGGAGTCATGTTT-3′). The amplified product was digested with AluI and the fragments visualized in a 6% polyacrylamide gel by silver staining .
24Sα ribosomal DNA gene PCR
The PCR analysis of the 24Sα rDNA gene (rDNA-PCR) described by Souto et al.  was used to discriminate the T. cruzi DTUs present in the IC from the groups of insects infected with two strains. The size of the amplified products of this gene for the T. cruzi strains belonging to the six DTUs is 110 bp (TcI, TcIII and TcV), 120 bp (TcIV) and 125 bp (TcII and TcVI), respectively [6, 45, 46]. This marker enables the three DTUs of the study present in the IC of the nymphs with mixed infection to be discriminated and identified. Amplification was performed with primers D71 (5′-AAGGTGCGTCGACAGTGTGG–3′) and D72 (5′-TTTTCAGAATGGCCGAACAGT–3′), and the amplicons were run in a 6% polyacrylamide gel and visualized by silver staining .
Determination of infectiousness and mortality rates
The pool of insects that presented a positive result in at least one of the methods applied (FE, DC and kDNA-PCR) in the excreta or IC was considered to be infected.
Deaths were recorded throughout the study period to determine the cumulative mortality rate in each experimental group.
Data were tabulated in a Microsoft Excel 2019 spreadsheet (Microsoft Corp., Redmond, WA, USA) and statistically analyzed using BioEstat 5.0 and GraphPad Prism 8.3.1 (GraphPad Software Incs., San Diego, CA, USA) softwares. Comparisons of means and standard deviations (SD) were performed for quantitative variables. Statistical comparisons were performed between the two triatomine species (R. robustus × R. pictipes) and between groups of pure and mixed infections containing the same strains (G1×G5, G1×G6, G2×G7, G2×G8, G3×G6, G3×G9, G4×G5, G4×G7, G4×G9), comparing groups two by two or all groups at the same time. Comparisons were also made between pure and mixed infections for each species and between species, both in the excreta and in the IC. The Mann-Whitney, Wilcoxon, Student's t and Shapiro–Wilk nonparametric tests were used to compare groups. For qualitative variables, analysis of variance and Bonferroni tests were used. The significance level adopted was 5%, with associations of P ≤ 0.05 considered to be significant.
Blood volume and mean number of blood trypomastigotes ingested
The pool of fifth-instar R. robustus and R. pictipes nymphs in all groups (G1–G9) showed a significant body weight gain (P = 0.007) following the blood meal (Table 1) with the nymphs of R. robustus having a significantly higher mean weight (P < 0.007) than those of R. pictipes (Table 1).
The R. robustus/TcIAM group (G1) showed the greatest increase in body weight, ingesting a mean of 1096 mg of blood, which is equivalent to 76,720 BT/µl, when compared between the nine groups for the same vector species and between vector species for the same experimental blood meal (Table 1). Among the R. pictipes groups, the greatest increase in body weight was recorded for the R. pictipes/TcIIPR group (G3), which ingested a mean of 687 mg of blood, corresponding to 48,090 BT/µl (Table 1). Despite the significant variation in weight gain between the vector species and even between the groups of the same species, we concluded that all insects were fed.
Fresh examination, differential count and kDNA-PCR positivity
Rhodnius robustus showed FE positivity rates (%+FE) in the excreta that ranged from 0.0% in G1 (TcIAM) and G6 (TcIAM+TcIIPR) to 30.0% in G4 (TcIVAM) (P = 0.0116), and in the IC from 0.0% in the same groups, G1 and G6, to 37.5% in G8 (TcIMG+TcIIPR), with no significant difference in the latter when IC was compared (Table 2). The DC positivity rates (%+DC) in the excreta ranged from 0.0% in seven of the nine groups (G1-G3, G6-G9) to 30.0% in G5 (TcIAM+TcIVAM) (P < 0.0001), and in the IC from 0.0% in G6 to 75.0% in G5; again, the difference was not significant for the IC samples. For kDNA-PCR, positivity rates varied significantly for both biological materials analyzed, demonstrating its greater sensitivity. In the excreta from R. robustus, the positivity rates ranged from 80.0% in G7 (TcIMG+TcIVAM) to 100.0% in six of the nine groups (G1, G3, G5, G6, G8 and G9) (P = 0.001), while in the IC, the positivity rates ranged from 50.0% in G2 (TcIMG) to 87.5% in four of the nine groups (G3-G6) (P = 0.039) (Table 2).
For R. pictipes, the %+FE in the excreta ranged from 0.0% in six of the nine groups (G2, G4, G5, G7-G9) to 20.0% in G6 (P = 0.001) and in the IC, with no significant difference, from 0.0% in G5 to 75.0% in G3 (TcIIPR) (Table 2). The %+DC varied significantly in the excreta (P = 0.002), from 0.0% in five of the nine groups (G2, G3, G7–G9) to 30.0% in G1, while kDNA-PCR positivity varied significantly in the IC (P = 0.012), from 37.5% in G8 and G9 to 100.0% in four groups (G3, G5–G7) (Table 2).
Comparisons of the mean number of parasitic forms in the FE of excreta and IC
The mean number of parasitic forms (PF) found in the FE of excreta and IC varied among the nine experimental groups, being significantly different (P < 0.05) for both biological materials of R. pictipes. For R. robustus, the mean number of PF ranged from 0.0 for G1 (TcIAM), G2 (TcIMG) and G6 (TcIAM+TcIIPR) to 1969.0 for G4 (TcIVAM) in the excreta, and from 0.0 for G1 and G6 to 6885.0 for G5 (TcIAM+TcIVAM) and 5535.0 for G7 (TcIMG+TcIVAM) in the IC (Fig. 2). In R. pictipes, no PF were observed in the excreta of six of the nine groups (G2, G4, G5–G7, G9), but the highest mean number of PF (2160.0) was recorded for G6. Of the three groups in which parasites were present in the IC, the mean number of PF in the IC of G3 (TcIIPR) (19,845.0) was significantly higher than that observed in both G8 (TcIMG+TcIIPR; 810.0 PF) and G9 (TcIIPR+TcIVAM; 675.0 PF) (Fig. 2).
The mean number of PF in the IC varied significantly (P = 0.0153) between the two triatomine species, with R. pictipes groups presenting the highest values, indicating that this species is more susceptible to T. cruzi infection than R. robustus, especially to the TcI strain from Amazonas, both alone and when associated with the TcII strain. The higher susceptibility to infection of R. pictipes in relation to R. robustus was also confirmed by the greater mean PF numbers in the TcII infections (Fig. 2).
After dissection of the insects' digestive tract, it was possible to observe the concomitant presence of MT, EP and SF in the DC (Fig. 3), regardless of the day of infection. The mean number of PF in the DC in the excreta of R. robustus ranged from 0.0 for seven of the nine groups (G1-G3, G6-G9) to 13.0 for G4 (TcIVAM) (P = 0.005), and in the IC, from 0.0 for G2 (TcIMG) and G6 (TcIAM+TcIIPR) to 40.0 for G4 (P = 0.007) (Table 3).
The mean number of PF in the DC for R. pictipes excreta ranged from 0.0 for six of the nine groups (G2–G4, G7–G9) to 6.0 for G1 (TcIAM) (P = 0.007), and from 1.0 for G5 (TcIAM+TcIVAM) to 189.0 for G4 in the IC (Table 4). For the experimental groups of R. robustus, in the first analysis of the excreta performed at 20 dpi, the SF and MT forms for G4 (TcIVAM) were visualized, and these were also visualized at 40 and 80 dpi (Table 3). In the case of mixed infections, MT was observed in the G5 group (TcIAM+TcIVAM) at 40 dpi (Table 3). In R. pictipes, the forms EP for G4 and MT for G5 were observed at 20 dpi, while at 60 dpi and 100 dpi, MT and SF were visualized for groups G1 and G6, respectively (Table 4).
Metacyclogenesis rates (%MC) in excreta for G4 (TcIVAM) and G5 (TcIAM + TcIVAM) of R. robustus were significantly higher, 53.8% (P = 0.005) and 50.0% (P = 0.004) respectively, than those in the other groups for this vector species. This demonstrates vector competence of R. robustus to TcIV, in both pure infection and mixed infection with TcIAM (Table 3). In the IC of this species, MT forms were found in both the pure infection groups (G1, G3, and G4) and mixed infection groups (G5, G7, G8, and G9) over the course of infection (Table 3).
MT forms were already observed at 30 dpi for G3 (TcIIPR) and G4, and the number of MT ranged from 0.0 for G2 (TcIMG) and G6 (TcIAM+TcIIPR) to 40.0 for G4. Rhodnius robustus was susceptible to pure infection with both TcII and TcIV as determined by the IC examination, and the highest percentages of MT forms recorded in this biological material were, in descending order, G5 (TcIAM+TcIVAM; 62.5%, P = 0.007) > G3 (TcIIPR; 44.4%, P = 0.005) > G4 (TcIVAM; 22.5%, P = 0.007) > G7 (TcIMG+TcIVAM; 21.1%, P = 0.006) > G8 (TcIMG+TcIIPR; 21.1%, P = 0.006) (Table 3).
Regarding R. pictipes, MT forms were observed in the excreta at 20 dpi for G5 (TcIAM+TcIVAM) (Table 4), indicating vector competence of this species for the Amazonas strains in mixed infection. MT forms were also observed in the excreta from G1 (TcIAM) at 60 and 100 dpi and from G6 (TcIAM+TcIIPR) at 80 dpi (Table 4). The %MC observed for these three groups (G1, G5 and G6) was 50.0%, which is significantly higher than the %MC in the other groups (P ≤ 0.005), demonstrating vector competence of this species for TcI from Amazonas both in pure and mixed infection with TcIV and TcII (Table 4). The highest percentages of MT forms (100.0%) were recorded for G5 (P = 0.003) and G9 (TcIIPR+TcIVAM) (P = 0.004) (Table 4). However, these two groups presented only one and two MT forms in the excreta, respectively.
The %MC in the groups of R. pictipes with a considerable number of PF in the excreta were, in descending order, 14.0% in G1 (TcIAM) > 12.5% in G8 (TcIMG+TcIIPR) > 6.3% in G6 (TcIAM+TcIIPR) > 5.0% in G3 (TcIIPR), indicating the vector competence of the species for TcI from Amazonas and TcII, both in pure and mixed infections (Table 4). In the R. pictipes IC, all three parasitic forms (EP, MT and SF) were observed for the four pure infection groups and only for G6 among the mixed infection groups (Table 4).
Trypanosoma cruzi genotyping
A RFLP-PCR of the COXII gene did not amplify T. cruzi DNA in any of the IC samples tested, despite numerous attempts, including restriction enzyme replacement. Thus, it was not possible to genotype the DTUs with this molecular marker for this type of biological material.
On the other hand, PCR genotyping of the T. cruzi 24Sα rDNA gene could be performed only for the IC samples (Fig. 4). In pure infections, the 110-bp band could be detected for TcIAM in the R. robustus IC (lane 19) and for TcIMG (lane 21) and the 125-bp band for TcIIPR (Lanes 23) in the R. pictipes IC (Fig. 4). In the mixed infection groups (G5-G9) of both Rhodnius species, DNA fragments of 120 or 125 bp were detected, characteristic of TcII and TcIV, respectively (Fig. 4).
Infectiousness and mortality
The results of the four techniques used demonstrated that the infectivity rates (%INF) of the four T. cruzi strains for R. robustus and R. pictipes, in pure and mixed infections, were 100.0% for all experimental groups, regardless of the biological material used in the analyses.
Mortality rates (%MOR) for the experimental groups with the two triatomine species ranged from 5.0% to 30.0%, with no significant difference. In pure infections, the highest %MOR recorded were for G1 and G2 (25.0% and 30.0%, respectively) of R. pictipes, and for R. robustus it was 20.0% for G1. The highest %MOR in mixed infections were 25.0% for G6 and G7 in R. pictipes and 20.0% for G8 in R. robustus, regardless of DTU and geographic origin (Table 5).
In the present study, the influence of the genetic diversity (DTU) of T. cruzi on the susceptibility to infection and vector competence of two different species of triatomines belonging to the genus Rhodnius was evaluated. Under controlled conditions, it was possible to observe T. cruzi infection by different strains in fifth-instar nymphs of R. robustus and R. pictipes. Furthermore, both Rhodnius species were susceptible (100.0% infectivity) to T. cruzi strains belonging to the TcI, TcII, and TcIV DTUs.
The amount of blood and BT ingested varied between the two triatomine species. Considering the groups of insects that ingested the highest amount of BT forms, the fifth-instar nymphs of R. robustus from G1 (TcIAM) ingested, on average, 76,720 BT, while those of R. pictipes from G3 (TcIIPR) ingested a mean of 48,960 BT. This difference in the volume of blood ingested and, consequently, in the amount of infective forms, is related to morphometric differences between the nymphs of the two species. Adult insects of the R. robustus species are known to be larger, measuring between 20 and 26 mm in length, while the adult insects of R. pictipes are between 18 and 22 mm in length . Barreto-Santana et al.  compared the blood intake between the different developmental stages of R. robustus and R. neglectus and reported that the highest intake was for the fifth-instar nymphs of R. robustus, while Rubio et al.  showed that fifth-instar nymphs of R. robustus ingest, on average, 337.19 mg of blood. However, for R. pictipes in the same nymphal stage, it has been reported that blood intake ranges from 127.40 to 199.50 mg [20, 32]. Therefore, the data in the present study show that R. robustus can ingest up to twice the volume of blood ingested by R. pictipes (730.0 vs. 465.0 mg), corroborating the results of other authors [20, 32, 48, 49].
The susceptibility to infection of R. robustus evaluated by the FE in the IC was higher for the TcIVAM strain, since the highest mean number of PF (1890.0) recorded was in the pure infection. Although the TcIAM strain originates from the same geographic area as R. robustus, PF were not observed in the IC of the nymphs infected by this strain. These data demonstrate that R. robustus is susceptible to infection by TcIVAM, but not to infection by TcIAM, suggesting that the genetic constitution of T. cruzi also influences this parameter. The mixed infection of both these Amazonas strains (G5) presented the highest number of PF in the IC (6885.0), suggesting a synergism between the two strains. Synergism seems to have also occurred between TcIVAM and TcIMG, which, when mixed (G7), had the second highest number of PF in the IC (5530.0). There was a predominance of TcIVAM when associated with TcIAM, TcIMG and TcIIPR, as observed in the rDNA-PCR genotyping that detected this DTU in the IC of R. robustus. These data show that the genetic lineage of the parasite influences the susceptibility to infection of the vector in the case of mixed infection. In the Brazilian Amazon, both TcI and TcIV have been isolated from naturally infected R. robustus and found to be associated with oral CD cases [28, 42, 50].
Rhodnius pictipes was observed to be susceptible to pure infection with the four T. cruzi strains studied (AM33, PR150, PR1256, and AM14), presenting the highest values in the mean number of PF in the IC of the entire study. The highest susceptibilities occurred both for the TcIAM (22,680.0 PF) and TcIVAM (10,665.0 PF) strains, from the Amazon region, and for the Paraná TcIIPR (19,845.0 PF) and Minas Gerais TcIMG strains (5670.0 PF). These data suggest that the susceptibility of R. pictipes to T. cruzi is also influenced by the genetics of the parasite, since this triatomine species, like R. robustus, was susceptible to the TcI strain from Minas Gerais. The number of PF observed in the IC of R. pictipes following infection with the mixed TcIAM and TcIIPR inoculum (17,145.0 PF) shows susceptibility but suggests a negative interaction between these two DTUs since the number of PF in the mixed infection was lower than the simple sum of the PF number for the pure infections. The lowest number of PF recorded for the other groups of R. pictipes in mixed infections with TcIMG+TcIVAM (2960.0 PF), TcIAM+TcIIPR (810.0 PF) and TcIIPR+TcIVAM (675.0 PF) also indicates antagonistic interactions. These values were lower−or even null (TcIAM+TcIVAM) in the case of G5−than those presented by the same strains alone in the pure infection groups (TcIAM, TcIMG, TcIIPR, and TcIVAM), suggesting partial or total inhibition of the parasite population in mixed infections. The genotyping data also showed that in mixed infections of both vector species in which TcI was present, this DTU was inhibited or eliminated by the other DTU and thus was not detected. A review of the literature showed that in nature, TcI has been the only DTU isolated from R. pictipes, as well as from the species Rhodnius pallescens, native to Colombia [7, 28, 51].
The vector competence, evaluated both by the presence and number of PF and by the %MC, in the excreta varied between the vector species and the T. cruzi strain. Based on the parameter “number of PF in the excreta” of R. robustus with pure infection, it was clear that the interactions between R. robustus and TcIVAM was greater (1969.0 PF) than that with all other groups, but no PF were observed in the R. robustus excreta for the TcIAM and TcIMG groups. These data demonstrate a greater influence of the parasite's genetics on the vector competence of this triatomine species; that is, in pure infections, R. robustus is able to eliminate greater amounts of PF from the TcIV strain in the excreta, but not from the TcI strains. The lowest values of the PF number in the excreta were recorded for TcI, regardless of geographic origin, in pure and mixed infections, except for the TcIAM+TcIVAM group (G5). Among the mixed infections in this vector, the infection with the TcIAM+TcIVAM strains had the highest number of PF in the excreta (560.0). However, this number was lower than the sum of the PF number of the pure infections with the same strains, suggesting that, although there is a negative interaction between the two Amazonas strains in R. robustus, leading to a reduction in the number of PF in the excreta, this species continues to eliminate PF along with the excreta, and may present vector competence for TcIAM+TcIVAM.
For R. pictipes, the results of the parameter “number of PF in the excreta,” indicate that PF elimination occurred only with TcI from Amazonas and TcII from Paraná, in both pure and mixed infections with these two strains. The highest PF values were observed in the excreta of this species, although the number of PF was lower than that observed in the IC; that is, for the TcI DTU, R. picitipes showed vector competence for the Amazonas strain, but not for the Minas Gerais strain, in addition to vector competence for TcII, whose geographic origin (Paraná) is different from the geographic area of occurrence of this vector species (R. pictipes, Amazon region). One implication of these experimental data is that this triatomine species could transmit TcII strains from another region when introduced in the Brazilian Amazon region.
Another important parameter to determine vector competence that also has an impact on the transmission of T. cruzi is the %MC. This metric determines the quality of the vector and also influences the transmission dynamics of the parasite; that is, the higher the %MC, the more effective the transmission of T. cruzi to the vertebrate host . The %MC must be determined both in the excreta and in the IC, because if infected insects are present during food processing, infective parasite forms in the excreta or the IC could contaminate the product when the insect is crushed. The results obtained for this parameter also suggest the influence of geographic origin on vector competence, since the highest %MC values were found in the excreta of R. robustus with TcIVAM (53.8%) and R. pictipes with TcIAM (50.0%) in pure infections, and in the IC of both R. pictipes (100%, only 1 MT form was observed) and R. robustus (62.5%) for the mixed infections of TcIAM+TcIVAM. An exception was the R. pictipes/TcIIPR+TcIVAM group which also had a %MC of 100% (only 2 MT forms were observed), even in the mixture a T. cruzi strain with a different geographic origin from the area where the vector species occurs. In the IC, the highest %MC (62.5%) was also recorded for R. robustus/TcIAM+TcIVAM. These data also suggest that these vector species showed high efficiency in transforming proliferative forms (EP) of T. cruzi into infective forms (MT). High efficiency in metacyclogenesis has also been observed in domestic species of Triatoma infestans, R. prolixus, and Panstrongylus megistus, where the %MC ranged from 60.0% to 70.0% for different DTU strains .
The interaction between the TcII strain from Paraná and the R. pictipes vector species in this study deserves mention. Even though this DTU is not frequently isolated in the Amazon region, the presence of this vector species has been reported beyond the borders of Brazil's Legal Amazon (states of Acre, Amazonas, Maranhão, Mato Grosso, Pará and Tocantins), such as the states of Piauí, Mato Grosso do Sul and Minas Gerais [32, 52]. The wide geographic distribution of this vector species increases the possibility of it encountering TcII strains in the Central-West, Southeast and South macro-regions of Brazil.
Our results show that strains of different DTUs tend to behave differently in both R. robustus and R. pictipes; that is, the interactions between the DTUs studied in these vectors differ in their ability to complete their biological cycle in the digestive tract. The best interactions occurred between T. cruzi strains and triatomine species of the same geographic origin, likely because the vector and the parasite are better adapted to each other due to a long period of co-evolution . Consequently, these parasites are able to become established and replicate efficiently in the vector and still produce infective forms, which is important in maintaining the life-cycle of the parasite in nature [26, 53, 54].
The genotyping of insect IC by rDNA-PCR showed that TcII and TcIV DTUs predominated (or overlapped TcI DTU) in the associations for both Rhodnius species. These results may be due the infective meal being performed on mice, where the host immune system, especially the cells of the mononuclear phagocytic system, could select parasite populations of one DTU to the detriment of another [55, 56]. That is, the parasite populations in the circulating blood of the mouse may be at different proportions and, consequently, the insect could feed and become infected with different proportions of each of the two strains . This selection of the T. cruzi population that occurs may also be related to intrinsic factors of triatomines (components present in saliva, lysozymes, defensins, etc.) that can inhibit the development of a certain genetic lineage of the parasite, as occurs with the Y (TcII) lineage in R. prolixus, where the components present in the insect's saliva inhibit the development of this strain [27, 57,58,59,60].
The parasitological techniques (FE and DC) used in this study, as well as kDNA-PCR, proved to be efficient for analyzing both biological materials. Among the techniques used, kDNA-PCR presented the highest sensitivity, being able to detect the DNA of the parasite both in the excreta and in the IC samples at greater proportions of the insects: from 50.0% (IC) to 100.0% (excreta) for R. robustus, and from 37.5% (IC) to 100.0% (excreta) for R. pictipes. This difference in kDNA-PCR sensitivity, observed between the two biological materials analyzed, may be associated with a greater presence of PCR inhibitors in the IC of these insects.
Genotyping by analysis of RFLP of the COXII gene, which involves cutting DNA fragments with the enzyme AluI, was also tested in the present study. However, this analysis showed partial or unspecific cleavage in the IC samples (data not shown). Our results differ from those reported by Sá et al.  for R. prolixus and suggest that both Rhodnius species studied may have components that inhibit the AluI activity. On the other hand, PCR of the 24Sα rDNA gene was able to detect and characterize genetic material only in the IC samples. This difference in detection capacity between kDNA-PCR and rDNA–PCR may be related to the amount of parasitic forms present in the samples and to the number of copies of the gene of interest. The kDNA minicircle is represented in thousands of copies, with an approximate size of 1.4 kb, and is considered to be a naturally amplified DNA [61,62,63].
This study showed that the two species of Rhodnius analyzed have vector capacity (susceptibility to infection and vector competence). Rhodnius robustus showed vector competence for pure infection of TcIVAM and mixed infection of TcIAM+TcIVAM, and R. pictipes showed vector competence for TcIAM+TcIVAM and TcIAM+TcIIPR. Early elimination of infective forms was observed for R. robustus, which increases its efficiency as a vector. Taken together, the data suggest that the genetics of the parasite and its geographic origin influence the susceptibility to infection and vector competence in pure and mixed infections of two triatomine species from the Amazon region.
Availability of data and materials
The datasets generated and/or analyzed during the current study are not publicly available (all data are shown in our results), but they are available from the corresponding author upon reasonable request.
Culture-derived metacyclic trypomastigotes
Discrete typing units
Liver infusion tryptose
Chagas C. Nova tripanozomiaze humana: estudos sobre a morfolojia e o ciclo evolutivo do Schizotrypanum cruzi n. gen., n. sp., ajente etiolojico de nova entidade morbida do homem. Mem Inst Oswaldo Cruz. 1909;1:159–218.
Coura JR, Borges-Pereira J. Chagas disease: what is known and what should be improved: a systemic review. Rev Soc Bras Med Trop. 2012;45:286–96.
WHO. Chagas disease (American trypanosomiasis). 2021. Available in: <https://www.who.int/health-topics/chagas-disease#tab=tab_1. Accessed Oct 2021.
Dias JCP, Ramos AN, Gontijo ED, Alejandro L, Shikanai-Yasuda MA, Coura JR, et al. II Consenso Brasileiro em Doença de Chagas, 2015. Epidemiol e Serviços Saúde. 2016;25:1–10.
Zingales B, Andrade SG, Briones MRS, Campbell DA, Chiari E, Fernandes O, et al. A new consensus for Trypanosoma cruzi intraspecific nomenclature: second revision meeting recommends TcI to TcVI. Mem Inst Oswaldo Cruz. 2009;104:1051–4.
Zingales B, Miles MA, Campbell DA, Tibayrenc M, Macedo AM, Teixeira MMG, et al. The revised Trypanosoma cruzi subspecific nomenclature: Rationale, epidemiological relevance and research applications. Infect Genet Evol. 2012;12:240–53.
Marcili A, Valente VC, Valente SA, Junqueira ACV, da Silva FM, Pinto AYDN, et al. Trypanosoma cruzi in Brazilian Amazonia: Lineages TcI and TcIIa in wild primates, Rhodnius spp. and in humans with Chagas disease associated with oral transmission. Int J Parasitol. 2009;39:615–23.
Zingales B. Trypanosoma cruzi genetic diversity: something new for something known about Chagas disease manifestations, serodiagnosis and drug sensitivity. Acta Trop. 2018;184:38–52.
Probst CM, de Melo MFAD, Pavoni DP, de Toledo MJO, Galdino TS, Brandão AA, et al. A new Trypanosoma cruzi genotyping method enables high resolution evolutionary analyses. Mem Inst Oswaldo Cruz. 2021. https://doi.org/10.1590/0074-02760200538.
Zhao Y, Galvão C, Cai W. Rhodnius micki, a new species of Triatominae (Hemiptera, Reduviidae) from Bolivia. Zookeys. 2021;1012:71–93.
Ramírez JD, Hernández C, Montilla M, Zambrano P, Flórez AC, Parra E, et al. First Report of human Trypanosoma cruzi infection attributed to TcBat genotype. Zoonoses Public Health. 2014;61:477–9.
de Oliveira J, Ayala JM, Justi SA, da Galvão JARC. Description of a new species of Nesotriatoma usinger, 1944 from Cuba and revalidation of synonymy between Nesotriatoma bruneri (Usinger, 1944) and N. flavida (Neiva, 1911) (Hemiptera, Reduviidae, Triatominae). J Vector Ecol. 2018;148:157.
Dorn PL, Justi SA, Dale C, Stevens L, Galvão C, Lima-Cordón R, et al. Description of Triatoma mopan sp. n. from a cave in in Belize (Hemiptera, Reduviidae, Triatominae). ZooKeys. 2018;775:69–95. https://doi.org/10.3897/zookeys.775.22553.
Lima-Cordón RA, Monroy MC, Stevens L, Rodas A, Rodas GA, Dorn PL, et al. Description of Triatoma huehuetenanguensis sp. n., a potential Chagas disease vector (Hemiptera, Reduviidae, Triatominae). Zookeys. 2019;820:51–70. https://doi.org/10.3897/zookeys.820.27258.
Poinar G. A primitive triatomine bug, Paleotriatoma metaxytaxa gen. et sp. nov. (Hemiptera: Reduviidae: Triatominae), in mid-Cretaceous amber from Northern Myanmar. Cretac Res. 2019;93:90–7.
Alevi KCC, de Oliveira J, da Silva RD, Galvão C. Trends in taxonomy of Chagas disease vectors (Hemiptera, Reduviidae, Triatominae): from Linnaean to integrative taxonomy. Pathogens. 2021;10:1627.
Nascimento JD, da Rosa JA, Salgado-Roa FC, Hernández C, Pardo-Diaz C, Alevi KCC, et al. Taxonomical over splitting in the Rhodnius prolixus (Insecta: Hemiptera: Reduviidae) clade: are R. taquarussuensis (da Rosa et al., 2017) and R. neglectus (Lent, 1954) the same species? PLoS ONE. 2019;14:e0211285.
da Rosa JA, Justino HHG, Nascimento JD, Mendonça VJ, Rocha CS, de Carvalho DB, et al. A new species of Rhodnius from Brazil (Hemiptera, reduviidae, triatominae). Zookeys. 2017;2017:1–25.
Abad-Franch F, Monteiro FA, Jaramillo ON, Gurgel-Gonçalves R, Dias FBS, Diotaiuti L. Ecology, evolution, and the long-term surveillance of vector-borne Chagas disease: a multi-scale appraisal of the tribe Rhodniini (Triatominae). Acta Trop. 2009;110:159–77.
Peixoto SR, Jurberg J. Biologia de Rhodnius stali, Lent, Jurberg & Galvão e Rhodnius pictipes Stål (Hemiptera, Reduviidae, Triatominae) em condições de Laboratório. EntomoBrasilis. 2014;7:193–8.
da Rocha DS, Jurberg J, Carcavallo RU, Presgrave OA, CunhaGalvão VC. Influência da temperatura e umidade no desenvolvimento ninfal de Rhodnius robustus. Rev Saude Publica. 2001;35:400–6.
Abad-Franch F, Lima MM, Sarquis O, Gurgel-Gonçalves R, Sánchez-Martín M, Calzada J, et al. On palms, bugs, and Chagas disease in the Americas. Acta Trop. 2015;151:126–41.
Coura JR, Junqueira ACV, Fernandes O, Valente SAS, Miles MA. Emerging Chagas disease in Amazonian Brazil. Trends Parasitol. 2002;18:171–6.
Garcia ES, Azambuja P. Development and interactions of Trypanosoma cruzi within the insect vector. Parasitol Today. 1991;7:240–4.
Alvarenga NJ, Bronfen E. Metaciclogênese do Trypanosoma cruzi como parâmetro de interação do parasita com o triatomíneo vetor. Rev Soc Bras Med Trop. 1997;30:247–50.
Dworak ES, De Araújo SM, Gomes ML, Massago M, Ferreira ÉC, de Toledo MJ, et al. Sympatry influence in the interaction of Trypanosoma cruzi with triatomine. Rev Soc Bras Med Trop. 2017;50:629–37.
Garcia ES, Genta FA, de Azambuja P, Schaub GA. Interactions between intestinal compounds of triatomines and Trypanosoma cruzi. Trends Parasitol. 2010;26:499–505.
Cordero-Montoya G, Flores-Villegas AL, Salazar-Schettino PM, Vences-Blanco MO, Rocha-Ortega M, Gutiérrez-Cabrera AE, et al. The cost of being a killer’s accomplice: Trypanosoma cruzi impairs the fitness of kissing bugs. Parasitol Res. 2019;118:2523–9.
Vivas RJ, García JE, Guhl F, Hernández C, Velásquez N, Ramírez JD, et al. Systematic review on the biology, ecology, genetic diversity and parasite transmission potential of Panstrongylus geniculatus (Latreille 1811) in Latin America. Mem Inst Oswaldo Cruz. 2021;116:1–18.
Catalá SS, Noireau F, Dujardin JP. Biology of triatominae. American Trypanosomiasis Chagas Disease. Amsterdam: Elsevier; 2017. p. 145–67.
de Abreu AP, Teston APM, Massago M, Lucas da Silva HF, Ferreira ÉC, de Fernandes N, et al. Experimental infection of Rhodnius robustus Larrousse, 1972 (Hemiptera, Reduviidae, Triatominae) with Trypanosoma cruzi (Chagas, 1909) (Kinetoplastida, Trypanosomatidae) IV. Exp Parasitol. 1927;2022:1–9.
Rocha DDS, Da Fonseca AH, Costa FA, Jurberg J, Galvão C. Desenvolvimento de Rhodnius pictipes Stal, 1872 alimentado através de membrana de silicone e em camundongos (Hemiptera, Reduviidae, Triatominae). Mem Inst Oswaldo Cruz. 1997;92:553–8.
Gomes ML, Toledo MJDO, Nakamura CV, Bittencourt NDLR, Chiari E, De Araújo SM. Trypanosoma cruzi: genetic Group with peculiar biochemical and biological behavior. Mem Inst Oswaldo Cruz. 2003;98:649–54.
Monteiro WM, Margioto Teston AP, Gruendling AP, dos Reis D, Gomes ML, Marques de Araújo S, et al. Trypanosoma cruzi I and IV stocks from Brazilian Amazon are divergent in terms of biological and medical properties in mice. PLoS Negl Trop Dis. 2013;7:e2069. https://doi.org/10.1371/journal.pntd.0002069.
Abolis NG, de Araújo SM, de Toledo MJO, Fernandez MA, Gomes ML. Trypanosoma cruzi I-III in southern Brazil causing individual and mixed infections in humans, sylvatic reservoirs and triatomines. Acta Trop. 2011;120:167–72.
Dias GBM, Gruendling AP, Araújo SM, Gomes ML, de Toledo MJO. Evolution of infection in mice inoculated by the oral route with different developmental forms of Trypanosoma cruzi I and II. Exp Parasitol. 2013;135:511–7.
Teston APM, Monteiro WM, Reis D, Bossolani GDP, Gomes ML, de Araújo SM, et al. In vivo susceptibility to benznidazole of Trypanosoma cruzi strains from the western Brazilian Amazon. Trop Med Int Heal. 2013;18:85–95.
Teston APM, de Fernandes NS, Abegg CP, de Abreu AP, Sarto MPM, Gomes ML, et al. Therapeutic effects of benznidazole in Swiss mice that are orally inoculated with Trypanosoma cruzi IV strains from the Western Brazilian Amazon. Exp Parasitol. 2021;228:108136.
Brener Z. Therapeutic activity and criterion of cure on mice experimentally infected with Trypanosoma cruzi. Rev Inst Med Trop Sao Paulo. 1962;4:389–96.
Camargo EP. Growth and differentiation in Trypanosoma cruzi. I. Origin of metacyclic trypanosomes in liquid media. Rev Inst Med Trop Sao Paulo. 1964;6:93–100.
Abegg CP, de Abreu AP, da Silva JL, de Araújo SM, Gomes ML, Ferreira ÉC, et al. Polymorphisms of blood forms and in vitro metacyclogenesis of Trypanosoma cruzi I, II, and IV. Exp Parasitol. 2017;176:8-15. https://doi.org/10.1016/j.exppara.2017.02.013.
Macedo AM, Martins MS, Chiari E, Pena SDJ. DNA fingerprinting of Trypanosoma cruzi: A new tool for characterization of strains and clones. Mol Biochem Parasitol. 1992;55:147–53.
Miyamoto CT, Gomes ML, Marangon AV, Araújo SM, Bahia MT, Lana M, et al. Trypanosoma cruzi: Sensitivity of the polymerase chain reaction for detecting the parasite in the blood of mice infected with different clonal genotypes. Exp Parasitol. 2006;112:198–201.
Sá ARN, Dias GBM, Kimoto KY, Steindel M, Grisard EC, Toledo MJO, et al. Genotyping of Trypanosoma cruzi DTUs and Trypanosoma rangeli genetic groups in experimentally infected Rhodnius prolixus by PCR-RFLP. Acta Trop. 2016;156:115–21.
Souto RP, Fernandes O, Macedo AM, Campbell DA, Zingales B. DNA markers define two major phylogenetic lineages of Trypanosoma cruzi. Mol Biochem Parasitol. 1996;83:141–52.
Lewis MD, Ma J, Yeo M, Carrasco HJ, Llewellyn MS, Miles MA. Genotyping of Trypanosoma cruzi: Systematic selection of assays allowing rapid and accurate discrimination of all known lineages. Am J Trop Med Hyg. 2009;81:1041–9.
Galvão C, Dale C. Chaves de identificação para adultos. Vetores da doença Chagas no Bras. Curitiba: Sociedade Brasileira de Zoologia, vol. 1, 2014. p. 171–208.
Barreto-Santana D, Starling J, Gurgel-Gonçalves R, Cuba CAC. Biologia comparativa e comportamento alimentar de Rhodnius neglectus e Rhodnius robustus (Triatominae) sob condições de laboratório. Rev Soc Bras Med Trop. 2011;44:490–5.
Rubio C, Moncada LI, Rojas MA, García A. Comportamiento de Rhodnius robustus Larousse, 1927 (Hemiptera, Reduviidae) durante su alimentación en condiciones de laboratorio. Biomedica. 2013;33:205–13.
dos Reis D, Monteiro WM, Bossolani GDP, Teston APM, Gomes ML, de Araújo SM, et al. Biological behaviour in mice of Trypanosoma cruzi isolates from Amazonas and Paraná, Brazil. Exp Parasitol. 2012;130:321–9.
Monteiro WM, Magalhães LKC, de Sá ARN, Gomes ML, de Toledo MJO, Borges L, et al. Trypanosoma cruzi IV causing outbreaks of acute chagas disease and infections by different haplotypes in the Western Brazilian Amazonia. PLoS ONE. 2012;7:e41284.
Lent H, Wygodzinsky P. Revision of the triatominae (Hemiptera, Reduviidae), and their significance as vectors of chagas’ disease. Bull Am Mus Nat Hist. 1979;163:123–520.
Pinto ADS, De Lana M, Bastrenta B, Barnabé C, Quesney V, Noël S, et al. Compared vectorial transmissibility of pure and mixed clonal genotypes of Trypanosoma cruzi in Triatoma infestans. Parasitol Res. 1998;84:348–53.
Pinto ADS, De Lana M, Britto C, Bastrenta B, Tibayrenc M. Experimental Trypanosoma cruzi biclonal infection in Triatoma infestans: detection of distinct clonal genotypes using kinetoplast DNA probes. Int J Parasitol. 2000;30:843–8.
Gazzinelli RT, Denkers EY. Protozoan encounters with Toll-like receptor signalling pathways: implications for host parasitism. Nat Rev Immunol. 2006;6:895–906.
Pena DA, Eger I, Nogueira L, Heck N, Menin Á́, Báfica A, et al. Selection of TcII Trypanosoma cruzi population following macrophage infection. J Infect Dis. 2011;204:478–86.
Coura JR, Viñas PA. Chagas disease: a new worldwide challenge. Nature. 2010;465:S6-7.
de Fuentes-Vicente JA, Gutiérrez-Cabrera AE, Flores-Villegas AL, Lowenberger C, Benelli G, Salazar-Schettino PM, et al. What makes an effective Chagas disease vector? Factors underlying Trypanosoma cruzi-triatomine interactions. Acta Trop. 2018;183:23–31.
Rodríguez-Ruano SM, Škochová V, Rego ROM, Schmidt JO, Roachell W, Hypša V, et al. Microbiomes of North American triatominae: the grounds for Chagas disease epidemiology. Front Microbiol. 2018;9:1–11.
Córdoba-Aguilar A. Chagas bugs and Trypanosoma cruzi: puppets and puppeteer? Acta Trop. 2020;211:105600.
Gomes ML, Macedo AM, Vago AR, Pena SDJ, Galvão LMC, Chiari E. Trypanosoma cruzi: Optimization of polymerase chain reaction for detection in human blood. Exp Parasitol. 1998;88:28–33.
Lukeš J, Lys Guilbride D, Votýpka J, Zíková A, Benne R, Englund PT. Kinetoplast DNA Network: evolution of an Improbable structure. Eukaryot Cell. 2002;1:495–502.
Klingbeil MM, Englund PT. Closing the gaps in kinetoplast DNA network replication. Proc Natl Acad Sci USA. 2004;101:4333–4.
The authors thank Dr. José Jurberg of the Laboratório Nacional e Internacional de Referência em Taxonomia de Triatomíneos do Instituto Oswaldo Cruz (IOC) /Fiocruz for providing the triatomines to the Parasitology Sector of the Departamento de Ciências Básicas da Saúde at the Universidade Estadual de Maringá.
Financial support was provided by: Coordenação de Aperfeiçoamento de Pessoal de Nível Superior-Brazil (CAPES) (Financing Code 001), the Fundação Araucária de Apoio ao Desenvolvimento Científico e Tecnológico do Estado do Paraná (10943812,251//2014) and the Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) (483469/2013–0).
Ethics approval and consent to participate
This work was approved by the Comissão de Ética no Uso de Animais of Universidade Estadual de Maringá (CEUA/UEM) (registration number 9659251017). The use of T. cruzi strains obtained from humans was approved by the Ethics Committees of the Fundação de Medicina Tropical Doutor Heitor Vieira Dourado (registration no. 360/07) and of UEM (registration no. 100/04 and 375/07).
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de Abreu, A., Lucas da Silva, H.F., Sarto, M.M. et al. Infection susceptibility and vector competence of Rhodnius robustus Larrousse, 1927 and R. pictipes Stal, 1872 (Hemiptera, Reduviidae, Triatominae) for strains of Trypanosoma cruzi (Chagas, 1909) (Kinetoplastida, Trypanosomatidae) I, II and IV. Parasites Vectors 15, 239 (2022). https://doi.org/10.1186/s13071-022-05350-3
- Chagas disease
- Experimental infection