Predicting how Leishmania will respond to control efforts requires an understanding of their transmission strategy. Using real-time quantitative PCR to quantify infectious metacyclic and non-metacyclic forms in mouse skin from single sandfly bites we show that most transmissions were highly enriched for infectious parasites. However, a quarter of sandflies were capable of transmitting high doses containing more non-infectious promastigotes from the vector’s midgut. Mouse infections replicating “high” to “low” quality, low-dose transmissions confirmed clear differences in the pathology of the infection and their onward transmissibility back to sandflies. Borrowing methods originally developed to account for exposure heterogeneity among hosts, we show how these high-dose, low-quality transmitters act as super-spreading vectors, capable of inflating Leishmania transmission potential by as much as six-fold. These results highlight the hidden potential of transmission of mixed Leishmania promastigote stages on disease prevalence and the role of dose heterogeneity as an underlying strategy for efficient transmission.
Leishmaniasis is a parasitic protozoal disease caused by the bite of an infected phlebotomine sandfly. It afflicts 12 million people in 98 countries and is responsible for 30,000–40,000 deaths with 1.2 million new infections annually1. A lack of a vaccine combined with a limited choice of drugs, which have toxicity issues and a growing incidence of drug resistance, place vector control as an important part of the future global elimination strategy2. Underpinning this is the need to understand the biology of Leishmania transmission and to model the transmission strategies of these parasites in both the lab and field2,3,4. Despite this need, we have poor information on the natural heterogeneity of Leishmania transmission, and currently no tools to measure transmission intensity in the field.
In the midgut of the sandfly, Leishmania develop into infective metacyclic promastigotes, a process termed metacyclogenesis. To achieve this, Leishmania must transform through various non-infectious stages of promastigotes (procyclic, nectomonad, leptomonad and haptomonad promastigotes). Collectively, their role is to replicate and colonize the sandfly forming a biological plug of parasites, which block the anterior midgut and modify the feeding behavior of the vector5,6,7,8. To do this they secrete filamentous proteophosphoglycan (fPPG), which condenses into the promastigote secretory gel (PSG), forcing the sandfly to regurgitate parasites during bloodfeeding9,10,11. One aspect of Leishmania transmission that has received very little attention is the composition of the parasite dose – the proportion of metacyclics delivered by bite. For leishmaniasis, this is a key question since parasites are likely to originate, via regurgitation, from the midgut where both metacyclics and non-metacyclics are embedded in PSG11. Currently, it is assumed that all infected sandflies transmit near-homogenous populations of metacyclics, based on a small number of studies which relied on determining the morphology of parasites recovered from capillary-feeding, membrane-feeding or from exudates squeezed from fresh bites9,12,13,14,15,16,17,18. Although informative, they do not fully replicate the natural feeding processes of the fly or the dynamic of deposition of the parasites into living skin.
Here we developed a real-time quantitative PCR (RTqPCR) strategy to quantify the number of metacyclic and non-metacyclic promastigotes within and delivered by individual sandflies to living mice. Contrary to current models, we show that there is heterogeneity in both the number and proportion of metacyclics transmitted by bite. Our study also shows that for Leishmania mexicana this infectiousness changes as the parasites mature in the vector Lutzomyia longipalpis, and can be affected by its feeding history and intrinsic factors during metacyclogenesis, such as the accumulation of the PSG plug. Strikingly, changes to the composition of the infectious dose from sandflies was shown to dramatically impact on the pathogenesis of cutaneous leishmaniasis and its infectiousness towards other sandflies. Mathematical modelling predicts that heterogeneity in dose composition may increase Leishmania transmission rate six-fold, highlighting that a proportion of sandflies act as super-spreading vectors.
RTqPCR to quantify metacyclics in sandflies and skin
Lutzomyia (Lu.) longipalpis sandflies were infected with Leishmania (L.) mexicana or Leishmania infantum, agents of zoonotic cutaneous and visceral leishmaniasis, and maintained until the infections had matured and undergone metacyclogenesis19,20. Individual flies were allowed to feed on the ears of BALB/c mice once and the bite site was analyzed by RTqPCR for the number of Leishmania parasites and the proportion of metacyclic promastigotes. Initially, a number of previously identified metacyclic-enriched Leishmania transcripts (Supplementary Table 1) were screened against, culture-derived non-infectious, L. mexicana and L. infantum nectomonads and infectious metacyclics (Fig. 1a, b). Following this, titration of L. mexicana and L. infantum metacyclics confirmed transcripts for small hydrophilic endoplasmic reticulum-associated protein (sherp)21,22,23 displayed sufficient specificity and sensitivity to discriminate and quantify the infective forms of these two species of Leishmania. In addition, metacyclics and nectomonads expressed similar amounts of small subunit ribosomal RNA (ssrRNA) transcripts (Supplementary Figure 1), confirming its ability to quantify infectious and non-infectious forms alike. As a negative control, neither of the promastigote forms expressed the amastigote-specific transcript, amastin (Supplementary Figure 1). By combining these parasites with a biopsy of mouse ear skin or an uninfected sandfly midgut we determined the abundance of ssrRNA and sherp transcripts and they formed our calibration curves for parasite and metacyclic quantification throughout the rest of the study. To determine the threshold sensitivity of detection of this method, we established a standard curve using serial 10-fold dilutions of L. mexicana or L. infantum parasites ranging from 106 to 1 parasite per reaction (Supplementary Figure 2 and Supplementary Table 2). Using ssrRNA, we were able to reliably detect down to 1 Leishmania cell per reaction for both species. Mean standard curves were calculated from five independent experiments in triplicate and was linear over the 7 log-dilutions of L. mexicana and L. infantum parasites with a correlation coefficient of 0.9927 and 0.9868, respectively. The ssrRNA and sherp RTqPCR proved highly reproducible over the entire range of parasite numbers and proportions of metacyclics, showing intra- and inter-assay coefficients of variation lower than 1.22% and 11.3%, respectively, and sensitivity to 1.4 pg Leishmania cDNA in as much as 2 μg mouse ear or 100 pg sandfly midgut cDNA (Supplementary Figures 2, 3, 4, 5 and Supplementary Tables 2, 3, 4, 5). Importantly, ssrRNA expression was very similar over the range of metacyclic proportions for all parasite numbers tested, confirming equal expression in non-infectious and infectious promastigotes (Supplementary Figure 3 and Supplementary Table 3).
To validate this method in sandflies we performed the sherp RTqPCR on sequential days of L. mexicana and L. infantum infection in Lu. longipalpis, and compared this to direct counting of promastigotes from midgut homogenates and determining the proportion of metacyclics from Giemsa-stained smears (Supplementary Figure 6a–d). The sherp RTqPCR showed close agreement with the established morphological method of quantifying metacyclics as the midgut infections matured. Going further, we tested the ability of the sherp RTqPCR to discriminate the non-infectious promastigote forms of L. mexicana and L. infantum from metacyclics obtained from infected sandflies. Amastigotes from infected mouse skin or spleens were used as negative controls (Fig. 1c, d). Collectively, these results show that for these species of Leishmania the combination of ssrRNA and sherp RTqPCR provides a robust method to discriminate and quantify metacyclics and non-metacyclics both in sandflies and in the skin following transmission. However, the use of the qPCR based on sherp expression may not be applicable for other Leishmania species or strains, and we would advise that prior validation is necessary before use.
Infected sandflies transmit highly enriched doses of metacyclics
Studies that have determined the number of Leishmania promastigotes delivered by individual sandflies have highlighted the large variability of parasite transmission19,24,25. In addition to determining the number of L. infantum and L. mexicana promastigotes delivered by individual infected Lu. longipalpis sandflies (the dose); we used our sherp RTqPCR to determine the metacyclic/non-metacyclic composition of each transmission. ssrRNA RTqPCR revealed that L. mexicana- and L. infantum-infected flies could transmit a mean 4111 and 268 promastigotes, respectively (Fig. 2a, d, Supplementary Table 6). Doses of L. infantum and L. mexicana displayed a distinct bimodal distribution; similar to other studies that have investigated Leishmania major transmitted by Phlebotomus papatasi20 or L. infantum transmitted by Phlebotomus perniciosus and Phlebotomus duboscqi21. Confirming these earlier reports, the majority of bites resulted in low doses, with 74% (47/62 bites) of L. infantum-infected flies and 58% (46/80 bites) of L. mexicana-infected flies delivering less than 102 or 103 promastigotes, respectively. Sherp RTqPCR revealed that in general Leishmania-infected flies delivered highly enriched doses of metacyclics, with an average of 88% L. infantum and 85% L. mexicana metacyclics transmitted to skin per bite. However, in these flies it was low-dose transmissions, comprising the majority of L. infantum or L. mexicana bites, that were the most enriched for infective forms, such that 83% L. infantum and 76% L. mexicana bites transmitting less than 102 or 103 parasites, respectively, contained an average 89% and 92% metacyclics (Fig. 2b–f). By contrast, high doses of these infections (i.e., > 103 parasites) contained proportionally less metacyclics (“metacyclic-poor”), delivering an average 63% L. infantum and 68% L. mexicana infective forms per bite.
To gain further insight into the relationship between the sandfly infection and both the quantity and quality of the infectious dose we applied a Gaussian mixture cluster analysis on log-transformed total parasite counts to a separate set of 35 L. mexicana-infected flies, which had their midgut loads determined immediately following the infectious bite. A sandfly’s pre-feed infection load was determined by combining the dose of parasites with the parasitaemia in the sandfly midgut24. This analysis detected four clusters with normal distribution and equal variance (Fig. 2g, Supplementary Table 7). Two clusters displayed a strong positive correlation between dose and midgut infection intensity and two that displayed a negative correlation. Interestingly, the flies in which the relationship between parasite load and transmitted dose inverted were those with the highest infections (geometric mean 1.41 × 106; compared to the other flies: geometric mean 4.23 × 104). Notably, these flies had atypically high infections but still in line with loads occasionally recorded from field-caught flies26,27. When the proportion of metacyclics in each dose was determined, this revealed that the vast majority of flies (91%, 21/23 flies) capable of transmitting low to intermediary doses of < 5 × 102 parasites, representing all flies from cluster 1, 3 and 4, deposited metacyclic-enriched doses of ≥ 75% metacyclics. These flies harbored low to intermediary (cluster 1) or very high (cluster 3 and 4) infection intensities. In contrast, poor-quality transmission ( < 75% metacyclics/bite) was almost an exclusive feature of cluster 2 flies, despite containing high infection levels and transmitting the highest doses (Fig. 2g, Supplementary Table 7).
As Leishmania transmission is likely to be by regurgitation, especially from heavily infected flies9,12,24, we next calculated the proportion of the original gut infection that was deposited with each bite (Fig. 2h, Supplementary Table 7). We found that the high-dose, poor-quality transmitters from cluster 2 disgorged the highest proportion of their infection (geometric mean 7.7 %). By contrast, those flies able to transmit low to intermediary doses exhibited consistently high-quality transmission and deposited a geometric mean of 2.42% of their infection. However, at the extreme end of the spectrum, flies with unusually high midgut infections of 105–106 parasites (from cluster 3 and 4) transmitted doses containing > 95% metacyclics but could only disgorge a geometric mean 0.008% of their initial load, and deposit low doses of parasites. For these flies, the relationship between sandfly infection intensity and the proportion of metacyclics in the transmitted dose (Fig. 2i) demonstrated that dose quality dropped rapidly when the sandfly infection reached 5.4 × 103 then steeply recovered when the infection reached 3.6 × 105 promastigotes per midgut (at 80% metacyclics per bite). This suggests that dose quality is highest during early metacyclogenesis or later when the infection is very large. In between, flies that harbour moderate infections are more likely to regurgitate higher doses containing proportionally more non-metacyclics.
Composition of the infectious dose changes during metacyclogenesis
Leishmania metacyclogenesis starts after the parasites detach from the sandfly midgut epithelium following bloodmeal defecation. For L. mexicana in Lu. longipalpis metacyclogenesis typically occurs from day 4 and reaches a plateau by day 8 post-infection (p.i.), achieving 40–60% of the total infection (Supplementary Figure 6a)8,20. To see if there was an optimal window of transmission we assessed L. mexicana transmission from Lu. longipalpis as the infections underwent metacyclogenesis from day 5–9 p.i. (Fig. 3). During this time, the infection level and proportion of metacyclics accumulated in midguts as expected (Supplementary Table 8), indicating that flies with atypically high infections, as experienced in Fig. 2g, h, were absent. In the bite, the numbers of promastigotes delivered increased 10-fold from day 5 to 7, and then dropped slightly from day 7 to 9 p.i. (Fig. 3a). Despite the low numbers of parasites, the majority (14/18 bites, 78%) of day 5 p.i. flies deposited highly metacyclic-enriched doses ( > 95%; Fig. 3b, c), which continued into day 7 p.i. (31/38 bites, 82%) except that the average dose and range of doses increased. As metacyclogenesis proceeded the proportion of flies transmitting less enriched doses (24/38 bites, 63%) became more apparent, such that metacyclic-poor transmissions ( < 75%) were only detected from day 9 p.i. flies. In this cohort, flies capable of transmitting large doses ( ≥ 103 promastigotes) were more prominent, representing an eighth of flies (Fig. 3b).
Increasing metacyclic purity with multiple successive bites
Leishmaniasis tends to be a focal disease, suggesting that there might be an influence of parasite infection on sandfly biting behavior4,28. Using the sherp RTqPCR we took the opportunity to examine the composition of the dose from multiple infective bites, taken in rapid succession from the same fly to assess the efficiency of transmission, which may occur in infection hot-spots. The quantity and composition of the first, fifth and tenth bites from 53 day 7 or 8 L. mexicana-infected Lu. longipalpis to the ears of BALB/c mice were investigated. To encourage multiple feeding, each fly was allowed to feed for 45 s, as this was roughly a fifth of the time required for infected Lu. longipalpis to take a full bloodmeal8. Figure 4 shows that there was 68% drop in the mean number of transmitted promastigotes (Fig. 4a) and metacyclics (Fig. 4b) between the first and fifth bites. Although the range of doses delivered by these flies was somewhat lower than the previous experiments (Fig. 2), this probably reflects the fact that these flies were allowed to feed for less time. By the tenth bite we observed a significant drop of 92% in the mean number of transmitted parasites (P < 0.05), and metacyclics compared to the first bite (Fig. 4a, b). However, proportionally, the number of bites containing highly enriched doses of metacyclics ( > 95%) rose sharply from 48% to 75%, between the 5th and 10th bite (Fig. 4c). These results demonstrate that infected sandflies remain infectious for many, consecutive, bites (up to ten and possibly beyond) and the quality of transmission may improve with each bite. This, combined with an increase in a sandfly’s feeding persistence during metacyclogenesis20, may promote the high efficiency of Leishmania transmission even if the population of infectious flies is low.
PSG blockage promotes more metacyclic deposition with multiple bites
Flies from the multiple bite experiments in Fig. 4 and another set of flies allowed to bite only once were dissected and processed to determine a number of parameters pertinent to infection and plotted against the proportion of transmitted metacyclics5,8,13,20,24,29 (Fig. 5).
Corroborating the work of Stamper and colleagues29 on L. major transmission from P. duboscqi, meta-analysis of L. mexicana infectious bites from Lu. longipalpis revealed that, overall, the proportion and total number of metacyclics per fly correlated with the proportion of metacyclics from flies transmitting their 1st and 10th infectious bite (Fig. 5a, b). The same association was also seen with the total parasite midgut burden (Fig. 5c). However, flies transmitting > 95% metacyclics displayed a greater spread of values, indicating that a proportion of flies with small or immature infections could also deliver high-quality doses, although the majority came from flies with large infections and higher proportion of metacyclics in their midguts. The sandfly infection parameter most closely associated with the proportion of metacyclics in the transmitted dose was the amount of PSG present in the midgut of flies delivering their 1st or 10th infectious bite (Fig. 5d). Interestingly, the multiple bite flies yielded a negative correlation between post-feed midgut PSG levels and the quality of the 10th bite, whereas bites from flies exposed only once to mice showed a strong positive correlation. Stomodeal valve distortion, linked to the accumulation of PSG and blockage of the anterior midgut returned a similar result (Fig. 5e), whilst the amount of blood obtained during the transmissions displayed a negative correlation for flies taking multiple bites and those fed once (Fig. 5f). Wing area, a commonly used proxy for (pre-bloodfed) dipteran body size30, did not return any correlation with the proportion of egested metacyclics, confirming that this was not a confounding factor in our study (Supplementary Figure 7).
Meta-analysis of the loss of metacyclics from sequential infectious bites, by comparing the slope between the first and last (10th) transmission, revealed that the amount of PSG blocking the sandfly midgut correlated with deposition of metacyclic forms (Fig. 5g). Collectively, these results indicate that, in addition to the proportion of parasites that have differentiated to the infectious metacyclic form, formation of the PSG blockage is an important component of vectorial competency and predictor of efficient transmission.
Dose composition influences leishmaniasis and onward transmission
To test the consequence of dose quality for infection of the mammalian host we mimicked high- to low-quality L. mexicana transmissions using 5 × 102 sandfly-derived metacyclics inoculated into the ear dermis of BALB/c mice on their own (high-quality, 100% metacyclic dose), or premixed with 2.5 × 102 or 5 × 102 sandfly-derived nectomonads (low-quality, 75% and 50% metacyclic doses). These infections used 5 × 102 promastigotes as this is close to the geometric mean dose of L. mexicana parasites delivered by Lu. longipalpis bite 7–8 days p.i. (Fig. 2a). In addition, a fourth group of mice received a total of 1 × 103 nectomonads and a fifth group 1 × 103 metacyclics only.
Infections from doses of 100% nectomonads confirmed that this stage of Leishmania is poorly infectious to mice compared to metacyclics (Fig. 6a, b). However, strikingly, infections incorporating nectomonads in the infectious inoculum (mimicking low-quality doses) caused exacerbated cutaneous pathology. Lesions evolved with faster kinetics compared to those infections from high-quality doses (Fig. 6a), resulting in much larger lesions. The final amastigote burdens revealed the advantage of a high-quality dose to the overall parasite infection in mice (Fig. 6b) as lesions resulting from 5 × 102, 100% metacyclics harbored an average of 3- or 15-fold more parasites compared to those initiated with 75% and 50% mix of metacyclics and non-infectious nectomonads, respectively (average amastigote burden: 2.2 × 105 vs. 6.8 × 104 (75%) 1.5 × 104 (50%)). To assess the transmission potential of these groups of lesions back to sandflies we allowed uninfected flies to feed on them immediately before the lesions were harvested. To reduce variability between the two groups, only flies with full bloodmeals were selected for analysis and maintained for 4 days p.i. In the Lu. longipalpis-L. mexicana vector-parasite model the 4th day of infection represents the population of parasites that have successfully survived bloodmeal digestion and defecation and are those that will colonize the rest of the fly for onward transmission8. The proportion of infected flies and midgut parasite loads revealed that lesions initiated with 100% L. mexicana metacyclics were significantly more infectious to Lu. longipalpis sandflies compared to those generated from various mixtures of infectious and non-infectious promastigotes (P < 0.005, Fig. 6c). Collectively, these data confirm that the composition of the transmitted dose is an important determinant of disease outcome and onward transmission.
Neutrophils and IL-1β expression are associated with enhanced pathology of cutaneous leishmaniasis31,32,33,34,35. To assess the contribution of non-metacyclics to lesion formation we employed a dermal air-pouch model of inflammation13. Air-pouches were inflated on the backs of mice and injected with either PBS or 5 × 102 sandfly-derived L. mexicana metacyclics on their own (100%) or premixed with 5 × 102 sandfly-derived nectomonads (50%). Cells migrating into the air-pouches were characterized by morphology, and the supernatants analysed for chemokines CCL3 and CXCL2 and the pro-inflammatory cytokine IL-1β by ELISA (Fig. 6d, e). We observed that more macrophages responded to air-pouches infected with 100% metacyclics compared to 50% metacyclics, with a corresponding higher secretion of the macrophage–attracting chemokine CCL3. Infections with nectomonads present resulted in more neutrophil than macrophage recruitment, although the numbers of both cell types were lower than their 100% metacyclic counterparts. To further investigate their association with natural infection, we determined the expression of these innate immune mediators in high dose bites (≥ 103 promastigotes) from day 8 p.i. L. mexicana-infected flies, separated into either high (> 95%) or low (< 95%) proportions of metacyclics in the infectious bite (Fig. 6f). In accordance with the air-pouch model, low-quality transmission associated with a higher expression of CXCL2 and IL-1β, and high-quality transmission associated with a higher expression of CCL3. More recently, IL-1β activity and neutrophil recruitment in skin was shown to be promoted by the introduction of sandfly-associated bacteria with the bite35. Using expression of 16S rRNA as a proxy for the presence of bacteria associated with the skin (from the skin and/or the sandfly), we show that low-quality transmissions resulted in more bacteria compared to high-quality ones, and was associated with higher expression of IGF-1, promoted by regurgitation of infection-enhancing PSG from high-dose transmissions36. Collectively, these findings demonstrate that the proportion of metacyclic and non-metacyclic forms in the infective dose influence the magnitude of lesion severity and onward transmission to sandflies.
Heterogeneity in dose increases Leishmania transmission potential
The potential epidemiological impact of transmission variability is made most transparent by accounting for it in calculations for the basic reproduction number (R0): a transmission metric that denotes the average number of secondary infections produced by a primary infection introduced into a susceptible population. In vector-borne disease systems it has been acknowledged for decades that some hosts are bitten more than others, and Dye and Hasibeder37 developed methods to account for this heterogeneity: R0 is inflated by the factor 1 + α, where α is the coefficient of variance squared. The coefficient of variance is calculated as the standard deviation for all observations in the sample divided by the mean. A comprehensive discussion of the theory behind this inflation factor, and its utility in analysing over-dispersed data, can be found here38.
In the current study, high variability was recorded for individual sand flies in the number of infective metacyclics they transmit in bites (Fig. 2a, d). We have previously shown that biting persistence increased linearly with metacyclic burden among sandflies20. Therefore, biting among the proportion of sandflies that are heavily infected with infective stages of parasite is intensified. Only with the quantitative methods presented in the current analysis is it possible to parameterize the coefficient of variance to allow for this inflation. The resulting effect on the R0 of L. mexicana is that it is increased more than 5-fold [1 + (9142/4416)2 = 5.3)] when this heterogeneity is incorporated, and for L. infantum, transmission potential is increased 6-fold [1 + (448/201)2 = 6.0)].
The composition of the dose of Leishmania promastigotes delivered by individual sandflies into the skin of a mammalian host has never been determined before. Here we design and validate a new approach to quantify and characterize Leishmania metacyclogenesis in sandflies and transmission to mice using RTqPCR of sherp gene expression. This advances existing qPCR methods that only quantify total numbers of Leishmania promastigotes19,24,25, as it allows the investigator to simultaneously assess the infectivity of sandflies and the quality of experimental transmission by determining the proportion of infectious metacyclics in the midgut and inoculated by each bite. Using this technique, we demonstrate that the majority (71–76%) of infected bites contained enriched doses of metacyclics (80–100%). However, a quarter (for L. mexicana) to a third (for L. infantum) of bites contained less than 75% metacyclics and for L. mexicana these were almost exclusively transmitted from flies harboring intermediary-large infections (104–3 × 105 parasites/midgut), accompanying the egestion of up to 35% of the midgut infection.
By analyzing the bites from flies as the infection progressed a window of optimal transmissibility opened midway through metacyclogenesis. This suggests that Leishmania transmission is more efficient from flies that have low-intermediary parasite burdens, which transmit lower doses but deliver bites more enriched for metacyclics. If this is the case, how can flies with immature infections (e.g., day 5 infections containing less than 10% metacyclics) transmit > 95% metacyclics? Previously, we have observed that metacyclics accumulate towards the ends of the PSG plug, in the anterior midgut and the stomodeal valve where transmission by regurgitation is more likely8. This points toward the possibility of an active form of selection taking place in the fly during transmission, enriching the bite for metacyclics - a hypothesis that remains to be explored in future studies.
In support of this, very large sandfly infections appeared to limit the size of the infectious dose but select for the deposition of metacyclics. In contrast, flies with intermediary infections tended to transmit larger doses of poorer quality, depositing larger proportions of their midgut infection, presumably through regurgitation of the PSG blockage and the parasites within. From this data, we extrapolate that for L. mexicana, ‘optimal’ transmission, containing high proportions of metacyclics, occurred when the fly had infections either below 5.4 × 103 or above 3.86 × 105 promastigotes per gut for doses of ≥ 80% metacyclics. A similar result was found when analyzing the correlates of high- and low-quality doses from infected flies fed once or multiple times, such that high-quality transmissions (> 95% metacyclics) resulted from a wide range of proportion or number of gut metacyclics, and flies with few gut metacyclics could also transmit a high-quality dose. This may also reflect the nature of the blockage in these infected midguts and the parasite’s interaction with it.
Proportionally, more non-metacyclics were transmitted by flies with large infections and they delivered the highest proportion of their midgut infection. Furthermore, blockage of the fly with PSG correlated closely with the dose quality of flies transmitting in their first bite, showing us that it is a strong selective force for the deposition of metacyclics. However, meta-analysis of multiple fed flies allowed to bite 10 times, suggests that lower PSG in the midgut post-feed reflects greater regurgitation of PSG during multiple feeding, resulting in metacyclic-enriched bites. This may be due to the fact that most of it is egested during low-quality previous transmissions where non-metacyclic forms (nectomonad and leptomonad promastigotes) appear to be immobilized within the PSG8,11. In later transmissions, when the PSG is depleted and/or solubilized in the midgut, it is likely that characteristics of the metacyclic promastigote, such as strong swimming, small body and long flagellum, could take over as determining factors in the composition of the dose.
In the present study, we observed that the parasite burden in the context of PSG amount in the sandfly midgut was a strong predictor of parasite dose and the number of transmitted metacyclics. However, this relationship broke down for the majority of our infected flies with mature intermediary-heavy infections, which passively regurgitated more non-metacyclics embedded within the PSG plug during their first bite. Nevertheless, this cohort of high-dose, low-quality transmitters are likely to be important to spread the infection since we have shown that these sandflies are more likely to deposit more infection-enhancing PSG9,13 and have increased feeding persistence, because of the higher amounts of PSG blocking their midgut20. Further, we may also expect these flies to deliver increasingly higher proportions of metacyclics with each successive bite as shown with our multiple bite experiments. Transmission heterogeneities such as these may have a large impact on R0 as they potentiate host contact and vector infectiousness39,40. By modelling the contribution of Leishmania dose heterogeneity and increased feeding persistence to transmission, we find that these flies can increase transmission potential by up to 6-fold. Inflated transmission potential derived from heterogeneous biting is more typically discussed in the context of hosts, whereby a small proportion of ‘attractive’ individuals are bitten more and contribute disproportionately to transmission39,40,41,42,43. Although mathematically analogous, being vector-centric, the heterogeneity in our analysis depicts a phenomenon that is distinct from these previous modelling studies.
Subclinical infections represent the majority of human and animal infections44,45. Our results show that low-dose, metacyclic-rich L. mexicana transmissions from the majority of infected Lu. longipalpis establish the host as an efficient reservoir of infection; similar to Kimblin et al24. In addition, we find that low-dose infections of mice that are metacyclic-rich generate minimal pathology yet establish a persistent population of parasites with high transmissibility back to sandflies. A recent study by Serafim and colleagues demonstrated that multiple bloodmeals resulted in larger infections with a higher proportion of metacyclics46. Importantly, they observed a 4-fold increase in lesion frequency on mice bitten by twice-fed L. major-infected P. papatasi compared to single-fed flies. The authors speculate that multiple bloodmeals are likely to result in a higher proportion of high-dose transmitters. Based on our results, we would predict that multiple bloodmeals would not only promote high doses but also the transmission of higher proportion of metacyclics. Taking our results and those of Serafim et al. together, the possibility of an enhanced presence of high-dose, metacyclic-rich transmitters following multiple bloodmeals may influence the epidemiology of leishmaniasis. This would result in more cases of disease with reduced severity, perhaps even asymptomatic infection, and result in more opportunities for new sandflies to pick up an infection. Recently, Doehl and colleagues found that outward transmission of subclinical Leishmania donovani infections in the skin of immunocompromised mice was best achieved if the distribution of parasites were patchy at both the macro-scale (over the body of the mouse) and micro-scale (within a patch); favoured by the pool-feeding nature of sandfly bloodfeeding47. Therefore, as sandflies tend to feed multiple times from hosts in close proximity4,28,48, which is likely to be exaggerated when the fly is infectious20, we would predict that heterogenous parasite transmission, acquisition, and the ability of multiple bloodmeals to enhance sandfly infectivity would combine to promote intense focal transmission.
Experimentally, the metacyclic-qPCR has provided new insight to Leishmania transmission and its impact on disease progression. Our findings indicate that heterogeneity in metacyclic promastigote exposure contributes considerably to heterogeneity in infection risk and variation in Leishmania transmission potential. Establishing the heterogeneity of the infectious inoculum and its effect on disease pathology will improve our understanding of the variability of natural transmission events.
Ethical statement for animal studies
All animal experiments were carried out in accordance with the UK Animal Scientific Procedure Act (ASPA) 1986, which transposes European Directive 2010/63/EU into UK national law.
The animal studies were approved by the UK home office in granting Project licence 70/8427 under the Animal Scientific Procedure Act and all protocols had undergone appropriate local ethical review procedures by the Animal welfare and Ethical Review Board (AWERB) of The London School of Hygiene and Tropical Medicine.
Leishmania culture and morphology
Leishmania mexicana (MNYC/BZ/62/M379) or L. infantum (syn. Leishmania chagasi) (MHOM/BR/76/M4192) were cultured as previously described8,17. All cultures were initiated with 1 × 106 skin lesion (L. mexicana) or splenic (L. infantum) amastigotes per ml from infected BALB/c mice. For L. mexicana and L. infantum nectomonad promastigotes were obtained from mid-logarithmic phase cultures (day 2 or 3) in M199 medium (Invitrogen, supplemented with 1% penicillin-streptomycin (v/v), 1 x BME vitamins (v/v), 10% heat-inactivated foetal calf serum (v/v)), pH 7.2 at 26 °C. Leishmania infantum, metacyclic promastigotes were purified from stationary phase M199 cultures (day 9–10) by differential centrifugation over a Ficoll gradient49. Leishmania mexicana metacyclics were obtained by passaging mid-log nectomonads into Grace’s insect culture medium (Invitrogen, supplemented as above), pH 5.5, 26 °C at 5 × 105 per ml, harvested 7–8 days later and purified over Ficoll. Promastigotes were washed extensively in PBS before use and morphologically assessed through measurement of parasites from Giemsa-stained smears8. In addition, their sensitivity to complement killing was determined in vitro by exposure to fresh 5% pooled human serum for 30 min at 34 oC, to ensure appropriate populations were used for real-time quantitative PCR (RTqPCR) and animal infections. Typically, cultured generated metacyclic promastigotes were 90–95% resistant to human serum. For infected sand fly midguts, formalin-fixed samples of parasites were counted using a Neubauer hemocytometer, and their developmental morphology assessed as above.
Five-day-old Lutzomyia longipalpis (Jacobina strain) female sandflies were infected with L. mexicana or L. infantum amastigotes through an artificial membrane feeding system at a density of 2 × 106 amastigotes per ml in heparinized, heat-inactivated pooled human blood. L. mexicana amastigotes were harvested from the rump lesions of female BALB/c mice, and L. infantum amastigotes were isolated from the spleens of female BALB/c mice20. Blood-fed flies were separated and maintained under a 12 h light:dark cycle at 26.5 °C, 80%–95% relative humidity, and supplied 25% (w/v) sucrose ad libitum. Flies were denied the opportunity to lay eggs to minimize post-oviposition mortality20, and all dissected flies with mature infections were observed to contain eggs.
Age- and weight-matched female BALB/c mice were used as the source of the blood meal in each experiment. Mice were anesthetized by intraperitoneal (i.p.) injection of 30 μl Ketaset/Rompun mixture (100 mg kg−1 and 10 mg kg−1 body weight) and placed into a 25 cm3 netted cage; their bodies were screened with netting except for their ears, or in some experiments, their right infected leg. Care was taken to keep the same orientation and position of the mice for each exposure. For infected bites to the ear, flies were released into the cage singly. A sandfly was removed and recorded as a “no-feed” when 5 min after release had elapsed without it initiating a feed. In the majority of experiments, flies that began feeding within this time were allowed to feed for 5 min before removal for analysis. In multiple bite experiments flies were allowed 45 s before they were interrupted by gently brushing the antennae20, forcing them to fully retract their mouthparts from the skin before initiating a new bite at a different site. Flies took their first bite on the right ear by covering the left ear with micropore surgical tape. After this bite the fly was removed and the surgical tape was swapped over to cover the right ear. The fly was then reintroduced into the cage and encouraged to take multiple feeds on the left ear. Repeating the procedure of removing the fly and swapping the surgical tape allowed the 5th and 10th bites to be taken from the right ear. For an overview of the process, please see Supplementary Figure 8. If a fly approached the same position of previous bites on the right ear their antennae were gently brushed to encourage them to bite another part of the ear. For all bite experiments, a detailed plan of the position of each bite was recorded and bites in the same position were not processed. At the end of the experiment, sandflies were transferred to a glass vial, knocked down on ice, and their midguts dissected to assess distension by measuring the diameter of the stomodeal valve. Guts were then homogenized in PBS to quantify the infection by direct counting, measure haemoglobin levels using Drabkin’s reagent (Sigma-Aldrich, UK)8 and determine the relative quantity of PSG by semi-quantitative dot blot using LT15, a monoclonal antibody, that recognises the galactose-phosphate-mannose repeats in Leishmania phosphoglycans9,10. To assess the transmissibility of ear lesions to uninfected sandflies (xenodiagnosis) 250 day 2–4 female sugarfed flies, starved overnight, were allowed to feed on groups of five anaesthetised, infected BALB/c mice screened with netting and micropore tape except for their infected right ear. Fully engorged flies that bloodfed on the infected lesion were transferred to another cage and maintained for 4 days, as above, before dissecting their midgut to assess their infection.
Infection of mice
Six- to 8-week-old female BALB/c mice were infected either by intradermal (i.d.) injection of 2.5 × 102–1 × 103 metacyclic promastigotes or nectomonad promastigotes in 10 μl via insulin needles into the dorsal surface of the right ear, as indicated. Lesion development was monitored by measuring the diameter of the swelling or lesion with Vernier callipers. At the end of experiments, mice were humanely euthanized, and parasite burdens in the ear determined by direct counting via hemocytometer13. All procedures involving animals were approved by a local Animal Welfare Committee and performed in accordance with United Kingdom Government (Home Office) and EC regulations. The distribution of values did not show evidence of non-normality using the Shapiro-Wilk test and therefore parametric analysis was performed (t tests). The null hypothesis was rejected if P < 0.05.
Infection of dermal air-pouches
A concentration of 3 ml of sterile air was injected i.d. into the backs of shaved BALB/c mice to inflate an air-pouch. Into each air-pouch a total of 1 × 103 L. mexicana promastigotes of varying proportions of metacyclics to non-metacyclics were injected in a total of 150 μl endotoxin-free PBS using a 27-gauge needle. At 48 h post-injection the cells from the air-pouch were recovered using a 5 ml ice-cold medium cavity lavage. Supernatant from the first 0.5 ml of the lavage was retained for cytokine and chemokine analysis and the cells combined with the following 4.5 ml of the lavage. The cells were concentrated to 0.5 ml by centrifugation (1800 rpm, 5 min) and live cells counted by diluting in trypan blue dye using a Neubauer improved haemocytometer. To determine the proportion of neutrophils and macrophage/monocytes by morphology, cells were concentrated on to slides using a Shandon cytospin 2 (500 rpm, 5 min) and stained with 10% (v/v) Giemsa’s stain.
Tissue preparation and RNA extraction
During transmission, a record was made of the feeding position of each fly on each ear. Following exposure, bites were recovered by means of a 2 mm diameter punch biopsy centered on the bite site (presenting as a small erythematous dot) and rapidly frozen on dry ice. This minimized and standardized the amount of host skin processed to improve detection of rarer parasite transcripts. Ear biopsies were stored at −80 °C until required. Ear tissue was fragmented using a MiniBeadBeater (1 min, 5000 rpm) in 500 µl of lysis buffer with Precellys ceramic 2.8 mm beads, as previously described50. Dissected sandfly midguts were directly added to 250 μl lysis buffer and dispersed by drawing up and down in a pipette. RNA isolation was performed on the homogenate with the RNeasy Plus Mini kit (Qiagen, Courtaboeuf, France), according to the manufacturer’s instructions and eluted into 30 µl of RNase free water. RNA quality and quantity were determined using Nanodrop (ThermoFisher Scientific).
Oligonucleotide primers and real-time quantitative polymerase chain reaction
A panel of parasite genes were chosen according to the different quantity of transcripts during the life cycle of Leishmania (Supplementary Table 1). qPCR was performed and analysed as previously described36. Nono and l19 were selected as the most stable reference genes for the BALB/c ears36,50 and MSLIST6001 was selected for Lu. longipalpis midguts51. Primer sequences are shown in the Supplementary Table 9.
Determination of L. mexicana and L. infantum transcripts by RTqPCR in samples
Serial 10-fold dilutions of L. mexicana and L. infantum metacyclic promastigotes (106 to 100) were combined with nectomonad promastigotes (95%, 85%, 75% metacyclics) with a quarter of a mouse ear from naïve BALB/c mice, or with an uninfected sand fly midgut. The Leishmania gene target (ssrRNA) was used to quantify the number of parasites52 and a linear regression for each standard curve was determined using the number of Leishmania parasites against the Ct values of ssrRNA50. The Leishmania metacyclic gene target (sherp) was used to quantify the number of metacyclic promastigotes. A linear regression for each standard curve was determined (i.e. number of Leishmania parasites vs. Ct of sherp) and the ratio metacyclic number/non-metacyclic number was used to determine the proportion of metacyclic promastigotes (Supplementary Figure 4). Transcripts were determined from whole infected sandfly midguts or from different promastigote stages harvested from pools of 50–200 infected sandfly guts. To obtain enriched populations of the different promastigote stages, guts were sampled at various times based on previous experience8,20 (stated in Fig. 1 legend). 1 × 107 cultured cells and 7 × 105–1 × 106 sandfly derived cells were tested per replicate after they had been washed three times in ice cold PBS, flash frozen in liquid nitrogen and stored at −80 °C until required.
Determination of bacterial and host transcripts by RTqPCR in skin
A 2 mm diameter biopsies of skin were used to sample bites as described above. For a number of mice, cytokine, chemokine and bacterial transcripts were determined using RTqPCR in parallel to ssrRNA and sherp analysis. Skin biopsies from the opposite, naïve ear were used as the negative controls. We used nono and l19 genes as housekeeping genes36. Primer information can be found in Supplementary Table 7.
Luminex of dermal air-pouch supernatants
The first 0.5 ml of dermal air-pouch supernatants were assayed for CCL3, CXCL2 and IL-1β using a Bio-Plex Mouse cytokine assay (Biorad) according to the manufacturer’s protocols and quantified using a Luminex® 200 System (Luminexcorp)36.
The p values were determined with GraphPad Prism software version 5.0. As the data was not normal (assessed by a Shapiro–Wilk normality test), the Mann–Whitney unpaired t-test was used to test the value statistical significance between groups for most experiments. Results from sequential bites from the same infected sandfly was analysed using a Wilcoxon paired test (*P < 0.05, **P < 0.005, ***P < 0.0005). All statistical tests were two-tailed. Linear correlation coefficients were generated with GraphPad Prism by Spearman-rank correlation to assess the association of parameters of sand fly infection on the composition of the dose.
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
All data generated or analysed during this study are included in this published article (and its supplementary information files).
Alvar, J. et al. Leishmaniasis worldwide and global estimates of its incidence. PLoS ONE 7, e35671 (2012).
Kamhawi, S. The yin and yang of leishmaniasis control. PLoS Negl. Trop. Dis. 11, e0005529 (2017).
Cameron, M. M. et al. Understanding the transmission dynamics of Leishmania donovani to provide robust evidence for interventions to eliminate visceral leishmaniasis in Bihar, India. Parasit. Vectors 9, 25 (2016).
Courtenay, O., Peters, N. C., Rogers, M. E. & Bern, C. Combining epidemiology with basic biology of sand flies, parasites, and hosts to inform leishmaniasis transmission dynamics and control. PLoS Pathog. 13, e1006571 (2017).
Bates, P. A. Transmission of Leishmania metacyclic promastigotes by phlebotomine sand flies. Int. J. Parasitol. 37, 1097–1106 (2007).
Sacks, D. & Kamhawi, S. Molecular aspects of parasite-vector and vector-host interactions in leishmaniasis. Annu. Rev. Microbiol. 55, 453–483 (2001).
Dostálová, A. & Volf, P. Leishmania development in sand flies: parasite-vector interactions overview. Parasit. Vectors 5, 276 (2012).
Rogers, M. E., Chance, M. L. & Bates, P. A. The role of promastigote secretory gel in the origin and transmission of the infective stage of Leishmania mexicana by the sandfly Lutzomyia longipalpis. Parasitology 124, 495–507 (2002).
Rogers, M. E., Ilg, T., Nikolaev, A. V., Ferguson, M. A. J. & Bates, P. A. Transmission of cutaneous leishmaniasis by sand flies is enhanced by regurgitation of fPPG. Nature 430, 463–467 (2004).
Ilg, T. et al. Purification and structural characterization of a filamentous, mucin-like proteophosphoglycan secreted by Leishmania parasites. J. Biol. Chem. 271, 21583–21596 (1996).
Stierhof, Y. D. et al. Filamentous proteophosphoglycan secreted by Leishmania promastigotes forms gel-like three-dimensional networks that obstruct the digestive tract of infected sandfly vectors. Eur. J. Cell Biol. 78, 675–689 (1999).
Shortt, H. E. & Swaminath, C. S. The Method of Feeding of Phlebotomus Argentipes with Relation to Its Bearing on the Transmission of Kala-azar. Indian J Med Res. 15, 827–836 (1928).
Rogers, M. et al. Proteophosophoglycans regurgitated by Leishmania-infected sand flies target the L-arginine metabolism of host macrophages to promote parasite survival. PLoS Pathog. 5, e1000555 (2009).
Warburg, A. & Schlein, Y. The effect of post-bloodmeal nutrition of Phlebotomus papatasi on the transmission of Leishmania major. Am. J. Trop. Med. Hyg. 35, 926–930 (1986).
Killick-Kendrick, R., Wallbanks, K. R., Molyneux, D. H. & Lavin, D. R. The ultrastructure of Leishmania major in the foregut and proboscis of Phlebotomus papatasi. Parasitol. Res. 74, 586–590 (1988).
Adler, S. & Ber, M. Transmission of Leishmania tropica by the Bite of Phlebotomus papatasii. Nature 148, 227 (1941).
Rogers, M. E., Corware, K., Müller, I. & Bates, P. A. Leishmania infantum proteophosphoglycans regurgitated by the bite of its natural sand fly vector, Lutzomyia longipalpis, promote parasite establishment in mouse skin and skin-distant tissues. Microbes Infect. 12, 875–879 (2010).
Killick-Kendrick, R. in Host-Parasite Cellular and Molecular Interactions in Protozoal Infections (Eds. Chang, K-P. & Snary, D.) 397–406 (Springer Berlin, Heidelberg, 1987).
Secundino, N. F. C. et al. The transmission of Leishmania infantum chagasi by the bite of the Lutzomyia longipalpis to two different vertebrates. Parasit. Vectors 5, 20 (2012).
Rogers, M. E. & Bates, P. A. Leishmania manipulation of sand fly feeding behavior results in enhanced transmission. PLoS Pathog. 3, e91 (2007).
Knuepfer, E., Stierhof, Y. D., McKean, P. G. & Smith, D. F. Characterization of a differentially expressed protein that shows an unusual localization to intracellular membranes in Leishmania major. Biochem. J. 356, 335–344 (2001).
Sádlová, J. et al. The stage-regulated HASPB and SHERP proteins are essential for differentiation of the protozoan parasite Leishmania major in its sand fly vector, Phlebotomus papatasi. Cell Microbiol. 12, 1765–1779 (2010).
Doehl, J. S. P. et al. Leishmania HASP and SHERP genes are required for in vivo differentiation, parasite transmission and virulence attenuation in the host. PLoS Pathog. 13, e1006130 (2017).
Kimblin, N. et al. Quantification of the infectious dose of Leishmania major transmitted to the skin by single sand flies. Proc. Natl Acad. Sci. USA 105, 10125–10130 (2008).
Maia, C., Seblova, V., Sadlova, J., Votypka, J. & Volf, P. Experimental transmission of Leishmania infantum by two major vectors: a comparison between a viscerotropic and a dermotropic strain. PLoS Negl. Trop. Dis. 5, e1181 (2011).
Reale, S. et al. Fluorescence-based detection of Leishmania infantum DNA in phlebotomus vectors. Ann. N. Y. Acad. Sci. 1149, 334–336 (2008).
Naiff, R. D. et al. Epidemiological and nosological aspects of Leishmania naiffi Lainson & Shaw, 1989. Mem. Inst. Oswaldo. Cruz. 86, 317–321 (1991).
Werneck, G. L. et al. The burden of Leishmania chagasi infection during an urban outbreak of visceral leishmaniasis in Brazil. Acta Trop. 83, 13–18 (2002).
Stamper, L. W. et al. Infection parameters in the sand fly vector that predict transmission of Leishmania major. PLoS. Negl. Trop. Dis. 5, e1288 (2011).
Siomava, N., Wimmer, E. A. & Posnien, N. Size relationships of different body parts in the three dipteran species Drosophila melanogaster, Ceratitis capitata and Musca domestica. Dev. Genes. Evol. 226, 245–256 (2016).
Charmoy, M. et al. The Nlrp3 inflammasome, IL-1β, and neutrophil recruitment are required for susceptibility to a nonhealing strain of Leishmania major in C57BL/6 mice. Eur. J. Immunol. 46, 897–911 (2016).
Fernández-Figueroa, E. A. et al. Disease severity in patients infected with Leishmania mexicana relates to IL-1β. PLoS. Negl. Trop. Dis. 6, e1533 (2012).
Santos, D. et al. IL-1β production by intermediate monocytes is associated with immunopathology in cutaneous leishmaniasis. J. Invest. Dermatol. 138, 1107–1115 (2018).
Gimblet, C. et al. Cutaneous leishmaniasis induces a transmissible dysbiotic skin microbiota that promotes skin inflammation. Cell Host. Microbe 22, 13–24.e4 (2017).
Dey, R. et al. Gut microbes egested during bites of infected sand flies augment severity of leishmaniasis via inflammasome-derived IL-1β. Cell Host. Microbe 23, 134–143.e6 (2018).
Giraud, E. et al. Leishmania proteophosphoglycans regurgitated from infected sand flies accelerate dermal wound repair and exacerbate leishmaniasis via insulin-like growth factor 1-dependent signalling. PLoS Pathog. 14, e1006794 (2018).
Dye, C. & Hasibeder, G. Population dynamics of mosquito-borne disease: effects of flies which bite some people more frequently than others. Trans. R. Soc. Trop. Med. Hyg. 80, 69–77 (1986).
Wilson K. et al. in The Ecology of Wildlife Diseases (Eds. Hudson, P., Rizolli, A., Grenfell, B., Heesterbeek, H. & Dobson, A.) (Oxford University Press, Oxford, 2002).
Woolhouse, M. Quantifying transmission. Microbiol. Spectr. 5, (2017).
Stone, C. M. & Chitnis, N. Implications of heterogeneous biting exposure and animal hosts on Trypanosomiasis brucei gambiense transmission and control. PLoS Comput. Biol. 11, e1004514 (2015).
Guelbéogo, W. M. et al. Variation in natural exposure to anopheles mosquitoes and its effects on malaria transmission. Elife 7, e32625 (2018).
Smith, D. L., Drakeley, C. J., Chiyaka, C. & Hay, S. I. A quantitative analysis of transmission efficiency versus intensity for malaria. Nat. Commun. 1, 108 (2010).
Onori, E. & Grab, B. Indicators for the forecasting of malaria epidemics. Bull. World Health Organ. 58, 91–98 (1980).
Quinnell, R. J. & Courtenay, O. Transmission, reservoir hosts and control of zoonotic visceral leishmaniasis. Parasitology 136, 1915–1934 (2009).
Ready, P. D. Epidemiology of visceral leishmaniasis. Clin. Epidemiol. 6, 147–154 (2014).
Serafim, T. D. et al. Sequential blood meals promote Leishmania replication and reverse metacyclogenesis augmenting vector infectivity. Nat. Microbiol 3, 548–555 (2018).
Doehl, J. S. P. et al. Skin parasite landscape determines host infectiousness in visceral leishmaniasis. Nat. Commun. 8, 57 (2017).
Bern, C. et al. Risk factors for kala-azar in Bangladesh. Emerg. Infect. Dis. 11, 655–662 (2005).
Späth, G. F. & Beverley, S. M. A lipophosphoglycan-independent method for isolation of infective Leishmania metacyclic promastigotes by density gradient centrifugation. Exp. Parasitol. 99, 97–103 (2001).
Giraud, E. et al. A combined luciferase-expressing Leishmania imaging/RT-qPCR assay provides new insights into the sequential bilateral processes deployed in the ear pinna of C57BL/6 mice. Parasitol. Int. 63, 245–253 (2014).
Hellemans, J., Mortier, G., De Paepe, A., Speleman, F. & Vandesompele, J. qBase relative quantification framework and software for management and automated analysis of real-time quantitative PCR data. Genome Biol. 8, R19 (2007).
Ranasinghe, S., Rogers, M. E., Hamilton, J. G. C., Bates, P. A. & Maingon, R. D. C. A real-time PCR assay to estimate Leishmania chagasi load in its natural sand fly vector Lutzomyia longipalpis. Trans. R. Soc. Trop. Med. Hyg. 102, 875–882 (2008).
E.G. and M.E.R. were supported by the BBSRC (David Phillips Fellowship awarded to M.E.R., BB/H022406/1). O.M. was supported by the Basque Government (Fellowship BF109.183). We thank Ms. Patricia Aiyenuro and Shahida Begum for support with the sandfly colony at LSHTM.
The authors declare no competing interests.
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Giraud, E., Martin, O., Yakob, L. et al. Quantifying Leishmania Metacyclic Promastigotes from Individual Sandfly Bites Reveals the Efficiency of Vector Transmission. Commun Biol 2, 84 (2019). https://doi.org/10.1038/s42003-019-0323-8
Frontiers in Cellular and Infection Microbiology (2019)
Trans-Atlantic Spillover: Deconstructing the Ecological Adaptation of Leishmania infantum in the Americas
Promastigote secretory gel from natural and unnatural sand fly vectors exacerbate Leishmania major and Leishmania tropica cutaneous leishmaniasis in mice