Article | Open | Published:

Mouse models of Loa loa


Elimination of the helminth disease, river blindness, remains challenging due to ivermectin treatment-associated adverse reactions in loiasis co-infected patients. Here, we address a deficit in preclinical research tools for filarial translational research by developing Loa loa mouse infection models. We demonstrate that adult Loa loa worms in subcutaneous tissues, circulating microfilariae (mf) and presence of filarial biomarkers in sera occur following experimental infections of lymphopenic mice deficient in interleukin (IL)-2/7 gamma-chain signaling. A microfilaraemic infection model is also achievable, utilizing immune-competent or -deficient mice infused with purified Loa mf. Ivermectin but not benzimidazole treatments induce rapid decline (>90%) in parasitaemias in microfilaraemic mice. We identify up-regulation of inflammatory markers associated with allergic type-2 immune responses and eosinophilia post-ivermectin treatment. Thus, we provide validation of murine research models to identify loiasis biomarkers, to counter-screen candidate river blindness cures and to interrogate the inflammatory etiology of loiasis ivermectin-associated adverse reactions.


Loiasis (tropical eye worm) is a parasitic helminth disease affecting ~13–15 million people in forested areas of Central and West Africa1,2. The disease is transmitted by blood-feeding Chrysops tabanid flies carrying the causative agent, the filarial worm Loa loa. Infectious stage L. loa larvae develop into mature adults that migrate within subcutaneous tissues and the sub-conjunctiva. Mating adult worms release thousands of microfilarial larvae (mf) daily into the circulation, which are transmitted to the vector upon taking a blood meal3. Loiasis is the cause of limb oedema (Calabar swellings) following death of adult worms4. Chronic infections cause renal, cardiac, pulmonary and neurological pathologies3,5,6 linked to excess mortality7. Loiasis is also an urgent global health problem, as severe and potentially fatal neurological serious adverse events (SAE) may occur in hypermicrofilaraemic patients (≥30,000 mf/ml blood) following annual mass drug administration (MDA) of ivermectin (IVM, Mectizan®) for the treatment of the related filarial disease, onchocerciasis (also known as river blindness)8. Below this hypermicrofilaraemic threshold, loiasis individuals remain at significant risk of developing non-neurological, febrile, temporarily debilitating AE following IVM treatment8,9. The two filarial infections overlap in Central Africa10. Social science investigations have identified perceived risk of loiasis AE as a major factor in persistent non-participation in onchocerciasis IVM MDA11. Because IVM MDA has to be delivered annually, at a coverage of 80%, for periods of 15 years or more, to prevent onchocerciasis transmission12, and because in loiasis-endemic Central African foci, elimination is not estimated to occur deploying this strategy until >204513, co-infection poses a significant barrier for onchocerciasis elimination programmes. There is a pressing need to develop new treatment strategies for both loiasis and onchocerciasis to de-risk AE occurrence in loiasis co-endemic areas and increase participation in river blindness elimination campaigns. Strategies include developing a safe drug cure, which selectively targets adult Onchocerca and/or Loa without inducing the rapid Loa microfilaricidal activity of IVM14 and/or accurately diagnosing loiasis hypermicrofilaraemic individuals at risk of adverse reactions in a test-and-not-treat with IVM strategy15.

L. loa naturally infects an endangered species of monkey, the drill (Mandrillus leucophaeus), endemic to Central Africa. As a surrogate non-human primate model, the life cycle of L. loa can be maintained via experimental infection of splenectomised baboons16,17, a model which has recently been utilised to initiate exploratory pathology studies of IVM-associated neurological SAE18,19. This model has also generated adult and mf parasitic stages for a range of ex vivo studies. However, throughput of the baboon model is severely constraining for anti-filarial drug research and to identify potential targets for adjunct therapies to prevent IVM SAE. There is currently no microfilaraemic small animal model of loiasis to use as a refinement to non-human primates for loiasis translational research whilst simultaneously increasing throughput of preclinical candidate evaluations. Recently, we identified that attenuated development of juvenile adult L. loa from infectious inoculates could be generated in selective immune knockout mouse strains with impaired interleukin-4, IL-5 and IL-13 signalling, providing proof-of-concept that targeting host-adaptive immunity could allow development of human Loa isolates in mice20. Further, we have recently established immunodeficient mouse models of related filarial infections (Brugia and Onchocerca) and implemented them as preclinical macrofilaricidal drug screens21,22,23,24,25.

Here, we address the current limitation in loiasis preclinical infection models by evaluating whether lymphopenic, immunodeficient mouse strains are susceptible to patent infection with L. loa. Further, we explore whether stage-specific, L. loa microfilaraemic mice can be established by blood infusion as a more rapid and facile model system for drug screening, including use of immunocompetent mice for the purposes of exploring inflammatory responses post-IVM treatment.


Lymphopenic γc-deficient mice are permissive hosts of L. loa

As with other human filarial parasites, fully permissive L. loa infections cannot establish in immunocompetent mice due to type-2 associated immunity21,26. Developing larvae can survive up to 2 months post infection in IL-4Rα−/−/IL-5−/− BALB/c mice, but sexual maturity and production of microfilariae (mf) is not evident in these selective type-2 cytokine deficient animals20. We have defined the minimum pre-patent period prior to mf release into blood as 5 months post infection with human strain L. loa larvae in baboons18. We therefore investigated the long-term parasitological success of L. loa infection in a panel of ‘severe-combined’ lymphopenic immunodeficient mice (Fig. 1). Moderate levels of pre-patent adult L. loa infection were evident in CB.17 (BALB/c congenic) SCID mice (8/9 mice infected, median % recovery of inoculate = 8.5, Fig. 1a) 3 months post infection. Most NOD.SCID mice had cleared infection at the same time point (2/6 mice infected), suggesting a background strain-dependent susceptibility in CB.17(BALB/c) versus NOD lymphopenic mice (Fig. 1a). However, deletion of the common IL-2/7 gamma chain (γc) on the NOD.SCID background rendered mice highly susceptible to infection at the pre-patent adult stage (73% median recovery, 4/4 mice infected, p < 0.01 when comparing NOD.SCIDγc−/− and CB.17 SCID mice, Kruskal–Wallis with Dunn’s post-hoc test, Fig. 1a). We therefore infected both NOD.SCIDγc−/− mice (commonly known as the NOD.SCID Gamma or NSG research model) and another compound immunodeficient lymphopenic mouse line on the BALB/c background, RAG2−/−γc−/−, and compared parasitological success at the time point of expected patency (5 months) with RAG2−/− γc-sufficient mice. Both compound gamma chain-deficient mouse lines supported survival of adult L. loa at +5 months (NOD.SCIDγc−/− 4/4 mice infected, 25.5% median recovery, BALB/c RAG2−/−γc−/− 9/9 mice infected, 13% median recovery). Conversely, all BALB/c RAG2−/− mice had cleared infection at 5 months (0/10 mice infected, p < 0.0001 when comparing BALB/c RAG2−/−γc−/− to BALB/c RAG2−/− mice, Mann–Whitney test, Fig. 1a). At this time point in both compound immunodeficient mouse strains, the majority of worms were found in the natural tissue niches of Loa adult stages, namely the subcutaneous and muscle fascia tissues (88 and 78% of total recovered worms in NOD.SCIDγc−/− and BALB/c RAG2−/−γc−/− mice, respectively, n = 4–11, Fig. 1b). Mature male and female worms were recovered, determined by marked difference in lengths (2.9 ± 0.3 cm males, vs. 4.5 ± 0.3 cm females) combined with distinct reproductive morphological characteristics, at a ratio of between 3:1 and 4:1 females per male (n = 4–11, Fig. 1c, d; Supplementary Fig. 1, Movie 1). Development of patency was apparent via identification of all embryonic stages within female uteri (n = 4–11, Fig. 1d) and release of motile mf ex vivo (Supplementary Movie 2). Further, microfilaraemias in BALB/c RAG−/−γc−/− mice 5 months post infection were apparent (Supplementary Fig. 1).

Fig. 1

Chronic L. loa infection can be achieved in lymphopenic mice deficient in the common gamma chain. a L. loa adult worm burdens at 3 and 5 months post infection in lymphopenic mouse strains with or without compound IL-2/7 gamma chain (γc) deficiency (3 months: CB.17 SCID (n = 11), NOD.SCID (n = 6), NOD.SCIDγc−/− (n = 4). 5 months: NOD.SCIDγc−/− (n = 4), BALB/c RAG2−/ (n = 10), BALB/c RAG2−/−γc−/− (n = 9 mice)). Plotted is percentage adult recovery of infectious inoculum for individual mice and median levels. b Tissue distributions of adult L. loa in NOD.SCIDγc−/− (n = 4) or BALB/c RAG2−/−γc−/− (n = 9) mice, 5 months post infection. Plotted is mean percentage of total yields per tissue site. c Sex ratio of adult L. loa in NOD.SCIDγc−/− (n = 4) or BALB/c RAG2−/−γc−/− (n = 9) mice, 5 months post infection. Plotted is percentage adult recovery of infectious inoculum for individual mice and median levels. d Representative photomicrographs of L. loa female (upper left and middle pictures) and male (upper right) worms recovered from an infected BALB/c Rag2−/−γc−/− mouse at 5 months post infection. u uterus, p uterine pore, c coiled microfilariae, m microfilariae, s spicule. Scale bar = 1 cm. The micrograph at the bottom represents an hematoxylin/eosin staining of a paraffin-embedded section of a L. loa female worm recovered 1 month post implant in a BALB/c Rag2−/− mouse. u uterus, e embryos, smf stretched microfilariae, cmf coiled microfilariae. Scale bar: 0.2 mm. e Adult worm yield 1 month post adult implants in NOD.SCIDγc−/− and BALB/c Rag2−/− mice, n = 3–5. f Microfilariae production 1 month post-adult implants in NOD.SCIDγc−/− (n = 3) or BALB/c Rag2−/− mice (n = 5). g Summary table of filariasis test strips (FTS) outcome when testing worms culture supernatants after overnight incubation at 37 °C (n = 3 cultures) and mice sera from selected infection conditions, (n = 3 naive mice, n = 5 BALB/c Rag2−/− mice 1 month post implantation, n = 10 all other mouse infections). h Og4c3 quantitative circulating antigen at 5 months post infection, (n = 10 BALB/c Rag2−/− or n = 9 BALB/c RAG2−/−γc−/− mice). Plotted is individual data and median levels. Significant differences between strains are determined by two-tailed Mann–Whitney (two groups) or Kruskal–Wallis with Dunns post-hoc tests (>two variables). Significance is indicated: *p < 0.05, **p < 0.01, ****p < 0.0001

Due to the high reproducible parasitological success of mature L. loa in compound deficient mice at 5 months post infection, we surgically implanted recovered female and male worms (n = 5 per sex) subcutaneously into NOD.SCIDγc−/− or BALB/c RAG2−/− recipient mice. Adult motility under the skin of recipient mice was frequently evident (Supplementary Movie 3). One month post L. loa adult implantation (6 months development from infectious stage larvae), viable males and females could be recovered, mainly from subcutaneous tissues, in both mouse strains (3/3 NOD.SCID γc−/− and 5/5 BALB/c RAG2−/− recipients, Fig. 1e; Supplementary Fig. 2 and Movie 4). Furthermore, females were reproductively active 1 month following implantation assessed by embryograms ex vivo (Supplementary Fig. 2) with 3/3 NOD.SCID γc−/− (mean 5980 ± 2240 mf/ml) and 3/5 BALB/c RAG2−/− (mean 874 ± 740 mf/ml) recipients displaying microfilariaemias by this stage (Fig. 1f).

We tested the utility of the loiasis mouse model to detect biomarkers of living L. loa adult infection by using two commercially available kits originally developed to specifically detect Wuchereria bancrofti circulating filarial antigens: the Alera Filarial Test Strip (FTS) and the TropBio Og4C3 immunoassay. Corroborating reported cross-reactivity of the FTS in recognising Loa specific secreted antigens27,28, we identified a strong positive signal in supernatants of both female and male Loa ex vivo cultures (Fig. 1g; Supplementary Fig. 3). When examining sera from mice infected with L. loa L3, we found that antigenaemia detection with FTS was reproducibly apparent, dependent on Loa adult infection status, but independent of the age of adult worm infection or microfilaraemic status. Negative serology results were recorded in all naive BALB/c RAG2−/− mice (0/3 mice tested) or in BALB/c RAG2−/− mice that had cleared L. loa at 2–5 months post infection (0/10 mice FTS positive at each time point). However, all BALB/c RAG2−/−γc−/− infected mice (10/10 mice, 2 or 5 months post infection) and all BALB/c RAG2−/− mice implanted with adult L. loa (5/5 mice, one month post implantation) were FTS positive (Fig. 1g; Supplementary Fig. 3). Additionally, all infection positive BALB/c RAG2−/−γc−/− mice (8/8 mice) but not infection negative RAG2−/− mice (0/9 mice) were seropositive for the distinct filarial adult antigen, Og4C3, 5 months after experimental infection (p < 0.0001, Mann–Whitney test, Fig. 1h).

Loa parasitaemias can establish in mice

Due to the complexity and long lead-time prior to emergence of microfilaraemias in experimental infections/implantations of immunodeficient mice, we assessed whether infusion with purified L. loa mf could establish stable parasitaemias as a more facile, stage-specific infection model. We also compared performance of immunocompetent versus immunodeficient mouse lines. After administering intravenous injections of 4 × 104L. loa mf through the tail vein, we observed that wild-type (WT) BALB/c mice had scant and transient microfilaraemias in peripheral blood up to 4 days post infusion (mean 48 ± 21 mf/ml, n = 8) after which time, no peripheral circulating mf were detectable (0/8 mice, Fig. 2a). Conversely, L. loa microfilariaemias were consistently identified in cardiac blood samples at termination, at 7 days post infusion, and at higher densities compared with peripheral parasitaemias (mean 1073 ± 503 mf/ml, n = 13, Fig. 2b). This indicated that L. loa mf sequestered in the cardiopulmonary circulation, with only a minor transient peripheral circulation. To test whether splenic secondary lymphoid tissue or global adaptive immune status exerted a role in limiting L. loa microfilaraemias in vivo, we compared parasitaemias in WT adult splenectomised or SCID mice post infusion with 4 × 104L. loa mf. Splenectomy of BALB/c mice allowed a significantly ~twofold higher cardiac microfilaraemia at 7 dpi versus WT mice (mean 1894 ± 411 mf/mL, p = 0.01, one-way ANOVA with Dunnett’s post-hoc test, n = 13, Fig. 2b) and L. loa mf persisted in peripheral blood (assessed until 8 dpi, Fig. 2a). In CB.17 SCID mice, peripheral parasitaemias were also consistently detectable (Fig. 2a, n = 8). SCID L. loa cardiac microfilaraemias were further elevated ~fourfold versus WT mice (mean 4562 ± 1098, p = 0.001, one-way ANOVA with Dunnet’s post-hoc test, n = 15, Fig. 2b), with cardiac parasitaemias consistent and stable over days 2–8 in a time course experiment (n = 4–8 per time point, Fig. 2c). Splenectomy of SCID mice did not further increase yields of microfilaraemias compared with SCID controls (Supplementary Fig. 4).

Fig. 2

L. loa microfilariaemias can be established in immunocompetent and immunocompromised mice. a Time-course of peripheral microfilariaemias in CB.17 SCID (n = 12), BALB/c WT adult splenectomised (spl.), n = 14 or BALB/c WT, n = 8 mice, 2–8 days following infusion with 40,000 purified L. loa mf. Plotted are mean ± SEM of time course data. b Level of L. loa microfilariaemia in cardiac blood in CB.17 SCID, n = 13, BALB/c WT spl., n = 13 or BALB/c WT, n = 15 mice 7 days post infusion with 40,000 purified L. loa mf. Plotted are individual data and means ± SEM. c Level of L. loa microfilariaemia in cardiac blood in groups of n = 4–8 CB.17 SCID microfilaraemic mice, evaluated at between 2 and 8 days following infusion with 40,000 purified L. loa mf. Plotted are individual data and means ± SEM. All data are derived from a single individual experiment (c) or pooled from two experiments (a, b). Significant differences are determined by one-way ANOVA with Dunnett’s post-hoc tests for >2 groups of log-transformed data (a, b) or Kruskal–Wallis with Dunn’s post-hoc tests, per time point (c). Significance is indicated: *p < 0.05, **p < 0.01, ***p < 0.0001, nd not different

Loa microfilaraemic mice respond to ivermectin

We have recently developed and implemented CB.17 SCID mouse models of lymphatic filariasis and onchocerciasis to evaluate candidate macrofilaricidal activities21,22,23,24,25. We have also demonstrated a rapid microfilaricidal response of IVM against circulating Brugia malayi mf in this research model21,24. Considering the advantage of a unified ‘pan-filarial’ research model to interrogate PK/PD relationships of candidate macrofilaricidal drugs, including off-target effects on Loa mf, and because the highest titres of Loa mf could be achieved in CB.17 SCID mice, we selected this lymphopenic mouse strain for validation assessments as a loiasis microfilaraemic counter-screening model. To this end, CB.17 SCID mice were infused with 4 × 104L. loa mf and treated with single-dose IVM or vehicle. IVM mediated a rapid clearance of mf at 2 days post treatment (92% mean cardiac load reduction versus vehicle, n = 4, Fig. 3a). This significantly increased to a 99% mean reduction versus vehicle at 7 days post treatment (Student's T test, p = 0.013, n = 6, Fig. 3a). Peripheral microfilaraemias were completely cleared in 5/6 mice following treatment at 5 dpi (Wilcoxon test, p = 0.031, Fig. 3b). These rapid IVM response dynamics mirrored the efficacy typically observed in both experimentally infected baboons and human patients3,19. The rapid in vivo microfilaricidal activity of IVM was not emulated following short-course oral treatments with either of the candidate macrofilaricide drugs, flubendazole or oxfendazole24,29, verifying a lack of off-target efficacy of these benzimidazole chemotypes against Loa microfilaraemias (Fig. 3c). Contrastingly, IVM efficacy against Loa mf was not emulated in vitro unless ≥ 2-day exposures exceeded, by 1000-fold, the typical peak plasma concentrations in vivo following oral dosing (set at 40 ng/ml, Supplementary Fig. 5). Similarly, the more potent macrocyclic lactone, moxidectin, failed to mediate any direct toxicity in vitro against Loa mf at physiologically relevant levels (Supplementary Fig. 5). The in vitro insensitivity of Loa mf to macrocyclic lactones was similar to that of the human filaria, Brugia malayi (Supplementary Fig. 5).

Fig. 3

Ivermectin mediates rapid microfilaricidal activity in L. loa microfilaraemic mice. a Level of microfilaricidal efficacy in CB.17 SCID mice, 2 days (n = 4) or 7 days (n = 6) post-single oral treatment with ivermectin (IVM), expressed as a percentage reduction in cardiac blood L. loa microfilariaemias from mean vehicle control levels. Plotted are individual data and means ± SEM. b Change in peripheral L. loa in CB.17 SCID microfilaraemic mice (n = 6), 5 days following vehicle or single IVM injection. Plotted are individual data. c Differential microfilaricidal efficacy in microfilaraemic CB.17 SCID mice of oral (n = 8) and parenteral (subcutaneous; s.c, n = 4) IVM dosing compared with macrofilaricidal benzimidazole drugs, flubendazole (FBZ, single dose, n = 5) or oxfendazole (OX-BZ, daily for 5 days, n = 5). Plotted are individual data and means ± SEM. d Microfilaricidal efficacy of parenteral IVM dosing (n = 5) versus vehicle (n = 4) in microfilaraemic splenectomised BALB/c mice. Plotted are individual data and means ± SEM. e Microfilaricidal efficacy of parenteral IVM dosing in microfilaraemic BALB/c mice (n = 8 per group) ± prior immune priming (2 weeks before treatment) with s.c. inoculations of 104 heat-killed L. loa mf or in vehicle controls (n = 7). Plotted are individual data and means ± SEM. Data are pooled or representative of two individual experiments. Significant differences are determined by Student's T test for two groups or one-way ANOVA with Dunnett’s post-hoc tests for >2 groups of log10 transformed data. Significant changes in paired data are tested by Wilcoxon Tests. Significance is indicated: *p < 0.05, **p < 0.01, ***p < 0.0001

Due to the stable parasitaemias evident in both splenectomised and non-splenectomised, immune competent BALB/c WT mice, we investigated whether IVM microfilaricidal efficacy was potentiated by host adaptive immune status. When microfilariaemic splenectomised BALB/c mice were treated with IVM, a similar degree of efficacy was observed compared with SCID mice (mean 98% reduced microfilaraemia, 7 days post treatment, p = 0.011, Student's T test, n = 4–5, Fig. 3d). Immune-priming BALB/c mice with subcutaneous inoculations of heat-killed L. loa mf 2-weeks prior to infusion and IVM treatment augmented the IVM treatment response (90% vs. 97% mean reduction in naive versus immune-challenged mice 7 days post treatment, n = 8 per group, one-way ANOVA followed by Dunnett’s post-hoc test, p < 0.05 versus p < 0.01 compared with respective vehicle controls, Fig. 3e). Together the data indicate that L. loa microfilaraemic mice display a typical rapid initial microfilaricidal drug response to IVM over the course of 7 days post treatment and efficacy remains intact in SCID or asplenic mice. However, we provide evidence that prior exposure to Loa mf antigens in immune competent mice can bolster the rapid efficacy of IVM.

Ivermectin treatment of L. loa induces type-2 inflammation

Taking advantage of stable parasitaemias over 7 days in WT mice following immune-priming with heat-killed L. loa mf, we undertook luminex bead-based array analysis of 32 serological cytokines/chemokines 2–7 days post-IVM treatment and compared responses to untreated immune-primed mice or immunologically naive mice that had received matching infusions of 4 × 104L. loa mf (n = 8 mice per group, Fig. 4). Analytes that were up or downregulated by more than twofold in immune-primed mouse groups ( + /− IVM treatment) versus naive mice 2 days following L. loa infusions were interleukins (IL)-4, 5, 10, 17, interferon gamma (IFNγ), CC-chemokine ligand 11 (CCL11; eotaxin 1) and CXC-chemokine ligand 5 (CXCL5, Fig. 4a). These analytes were then examined in statistical models to determine significance of fold-changes following immune-priming and IVM treatment. Whilst immune-priming alone induced significant elevations in circulating interleukins (IL)-4 and IL-5 2 days following mf infusions compared with control mice (mean 3.9 ± 0.8 vs. 1.3 ± 0.3 pg/ml, p < 0.05 and 67 ± 13.9 pg/ml vs. 13.5 ± 1.5, p < 0.01), the magnitude of the IL-4 and IL-5 response was bolstered following IVM treatment (mean 5.0 ± 0.5 pg/ml, p < 0.01 and 151.2 ± 32.5 pg/ml, p < 0.001, one-way ANOVA followed by Dunnett’s post-hoc tests, Fig. 4b). Levels of IL-10 and IFNγ were only significantly elevated in the circulation of immune-primed plus IVM-treated microfilaraemic mice compared with controls (mean 25.5 ± 2.3 vs. 13.3 ± 1.1 pg/ml, p < 0.05 and 107.0 ± 15.9 vs. 45.4 ± 7.5 pg/ml, p < 0.01, one-way ANOVA followed by Dunnett’s post-hoc tests or Kruskal–Wallis test followed by Dunn’s post-hoc tests, respectively, Fig. 4b). Due to augmented efficacy of IVM after 7 days in immune-primed mice (Fig. 3), we examined the change in inflammatory responses that were initially up or downregulated post-IVM treatment between D2 and D7 post treatment. Levels of circulating IL-4 and IL-5 were not altered by D7, whereas IL-10 (mean 16.7 ± 2.9 vs. 25.5 ± 2.3 pg/ml, p = 0.036, Wilcoxon test), IFNγ (mean 3.7 ± 0.5 versus 107.0 ± 15.9 pg/ml, p = 0.008, Wilcoxon test) and IL-17 (mean 3.3 ± 0.8 vs. 6.5 ± 1.4 pg/ml, p = 0.039, Wilcoxon test) all significantly had decreased by this time point post-IVM treatment (Fig. 4c). Contrastingly, circulating levels of CCL11 had increased on average by > fourfold between D2 and D7 post-IVM treatment (1993 ± 134.4 vs. 450.8 ± 96.5 pg/ml, p = 0.008, Wilcoxon test). Therefore, a type-2 ‘eosinophilic-like’ inflammatory signature was evident in immunocompetent, antigen-experienced animals 7 days following treatment with IVM. Differential white blood cell counts were compared at baseline and D2 in individual mice. Both monocyte and neutrophil proportions were elevated in the blood of all groups 2 days after infusion with 4 × 104L. loa mf (3.8 ± 0.6, 9.8 ± 0.8 or 6.2 ± 3.3 mean fold increases in monocytes, 4.7 ± 0.5, 2.3 ± 0.3 or 3.0 ± 0.5-fold-increases in neutrophils, for untreated, immune-primed + untreated and immune-primed + IVM-treated mice, respectively, n = 5/group, all p < 0.05, paired T test, Fig. 5a). Contrastingly, the eosinophil white blood cell compartment was significantly elevated 2 days following L. loa infusion in IVM-treated mice only (3.1 ± 0.6 mean fold increase, p = 0.038, n = 5, paired T test, Fig. 5a). Tissue granulophilia was then measured within secondary lymphoid tissue or body cavities of L. loa microfilaraemic mice 7 days after infusion and IVM treatment, compared with untreated controls (Fig. 5b, c). In splenic tissues, a marked increase in eosinophils were apparent, associated with vasculature of the red pulp, in IVM-treated, immune-primed mice, compared with controls (2.1 ± 0.1 or 1.8 ± 0.05 mean fold change compared with naive or immune-primed sham-treated controls, respectively, n = 5, p < 0.001 one-way ANOVA with Dunnet’s post-hoc test, Fig. 5b; Supplementary Fig. 6). At the same time point, within the peritoneal cavity, a significant, eosinophil-specific granulocyte exudate was manifest in immune-primed + IVM-treated mice compared with sham-treated controls (1.0 ± 0.15 × 105 vs. 0.32 ± 0.06 × 105, p < 0.05, n = 5, one-way ANOVA with Dunnet’s post-hoc test, Fig. 5c; Supplementary Fig. 7). These data indicate that IVM treatment responses culminate in a significant increased myelopoiesis and generalised tissue recruitment of eosinophil granulocytes in immune-primed L. loa microfilaraemic mice.

Fig. 4

Type-2 systemic inflammation is evident post-ivermectin treatment of L. loa microfilaraemic mice. a Plasma cytokines/chemokine changes 2 days post infusion with 40,000 purified L. loa mf into BALB/c mice with prior immune-priming via s.c. inoculations of 1 × 104 heat-killed L. loa mf and either IVM 5 mg/kg (n = 8) or sham-treatment s.c. at the point of infusion (n = 8). Plotted is median fold change compared with non-immune primed, sham-treated L. loa microfilaraemic controls (n = 7). Colour scale depicts<−10 (dark blue) to >10 (dark red) fold difference with white being 1 (i.e., no difference). b Cytokines/chemokines with ≥twofold increase or decrease following immune-priming (n = 8) and/or immune-priming + IVM treatments (n = 8) compared with non-immune primed, sham-treated L. loa microfilaraemic controls (n = 7). Data plotted are individual data and means ± SEM. Significant differences are determined by one-way ANOVA with Dunnetts post-hoc tests of either raw or log-transformed data (IL-4, 5, 10, CCL11, CXCL5) or Kruskal–Wallis tests with Dunns post-hoc tests (IFNg, IL-17). c Changes in circulating cytokine/chemokine levels between 2 and 7 days post-IVM treatment in immune-primed L. loa microfilaraemic mice (n = 8). Plotted are individual data. Significant differences are determined by paired Student's T tests (IL-4, -5, -10) or Wilcoxon tests (IFNg, CCL11, CXCL5, IL-17). All data are pooled from two individual experiments. Significance is indicated: *p < 0.05, **p < 0.01. ***p < 0.001

Fig. 5

Ivermectin treatment induces eosinophilia in L. loa microfilaraemic mice. a Differential white blood cell counts determined by blood thin smear and MGG staining at baseline or 2 days post infusion with 40,000 purified L. loa mf into BALB/c mice ± prior immune-priming with s.c. inoculations of 1 × 104 heat-killed L. loa mf and sham or IVM 5 mg/kg treatment s.c. at the point of infusion (n = 5 mice per group). Proportions of basophils, eosinophils, monocytes and neutrophils were enumerated per 200 leucocytes per slide. Data plotted are specific cell proportions of total leucocytes (%) of individual mice and mean ± SEM. b Eosinophil counts in the red pulp, vasculature, white pulp marginal zones and germinal centres in sections of spleen 7 days post infusion with 40,000 purified L. loa mf into BALB/c mice ± prior immune-priming with s.c. inoculations of 1 × 104 heat-killed L. loa mf and sham or IVM 5 mg/kg treatment s.c. at the point of infusion (n = 3 mice per group). Plotted is mean counts for 10 quadrants of 120 µm x 200 µm per splenic zone per mouse, and mean ± SEM per group. c Eosinophil and neutrophil enumerations within peritoneal exudate cells acquired by flow cytometry, 7 days post infusion with 40,000 purified L. loa mf into BALB/c mice ± prior immune-priming with s.c. inoculations of 1 × 104 heat-killed L. loa mf and sham or IVM 5 mg/kg treatment s.c. at the point of infusion (n = 5 mice per group except sham group, n = 6). Plotted is individual data and mean ± SEM. Significant changes in paired data is tested by T test (a). Significant differences for three independent groups are determined by one-way ANOVA with Dunnett’s post-hoc tests (b, c). Significance is indicated: *p < 0.05, **p < 0.01, ***p < 0.001


There is renewed investment in developing repurposed, reformulated or new chemical entity small molecule compounds as macrofilaricides for the priority neglected tropical disease, onchocerciasis14,30. A safe, short-course macrofilaricidal agent without significant direct, rapid toxicity against circulating L. loa mf would be a solution to the spectre of IVM-associated SAE, which is currently contributing to extended global elimination timeframes far beyond the 2025 target in countries where loasis is endemic13. Whilst we have made recent advances in in vitro culture screening systems for loiasis, including mf screens31,32, the standard microfilaricidal agents: IVM, the related macrocyclic lactone, moxidectin and the piperazine derivative, diethylcarbamazine (DEC), are inactive in vitro against a range of filarial mf at concentrations known to induce efficacy in vivo33,34 (Supplementary Fig. 4). Host-directed factors are therefore speculated to be necessary for IVM efficacy, and DEC has been demonstrated to influence host innate inflammation33,34. Due to the current limitations in in vivo models of loiasis, our primary goal was to establish a mouse research model that could accurately evaluate efficacies of candidate macrofilaricidal drugs on various Loa life cycle stages, namely developing larvae or adults in subcutaneous tissues and mf in circulation.

Our results demonstrate that development of fecund adult Loa infections in the natural parasitic niche can be reproducibly achieved in compound immunodeficient, lymphopenic mice lacking the common gamma chain (γc) cytokine signalling pathway. Contrastingly, following maturation, adult Loa survival was not dependent on γc signalling, determined by recovery of mf-producing adult parasites 1 month post implantation in γc-sufficient SCID mice. A number of cytokines (IL-2, IL-4, IL-7, IL-9, IL-15 and IL-21) signal via this shared receptor chain35. This suggests that facets of the murine innate immune system require one or more of the γc cytokine pathways, either during haematopoiesis or in response to infection to control loiasis throughout the L3-L4-L5 development and growth phase. Innate lymphoid cells (ILC) are known to be important innate immune cells, which require γc-dependent cytokine signalling for haematopoietic development36. Because specific ILC sub-sets, namely natural killer (NK) cells and ILC2, expand and are associated with immune control of specific nematode infections, including experimental filarial infections36,37,38,39, further research is required to determine mechanistic roles for these cell types in the innate control of developing L. loa larvae in lymphopenic strains of mice.

The establishment of an adult loiasis research model will be of use in preclinical assessments of candidate macrofilaricides targeting Loa and the ability to implant defined burdens of Loa male and females prior to drug testing will aid accuracy of readouts. The model is thus ready to test treatment responses to ‘reference’ macrofilaricides, such as flubendazole, and to scrutinise whether dose alterations of human registered drugs (e.g., albendazole) or re-purposing the veterinary agents: emodepside or oxfendazole, can mediate substantial and selective macrofilaricidal activities against L. loa in vivo. Because Loa circulating glycoproteins could be readily detected by commercial filarial immunodiagnostic tests in both pre-fecund and fecund Loa infected mice, this research model could also be readily applied in the preclinical discovery of Loa adult biomarkers and evaluation of specific Onchocerca candidate biomarkers currently in development as potential point-of-care diagnostics40,41. Beyond translational research, the murine model will be of benefit to basic parasitological researchers by facilitating a convenient, abundant source of all mammalian life cycle stages of Loa parasites for molecular and genomic studies as an alternative to non-human primate (NHP) usage.

The more facile approach of infusing purified mf directly into venous blood generated similar levels of parasitaemias as observed post-adult implantations, in both immunodeficient and immunocompetent mice. No model supported ‘hypermicrofilariaemias’ in the peripheral circulation, but displayed between 102 and 104 mf/ml rapidly sequestering in the cardiopulmonary circulation following 4 × 104 mf infusions. This may reflect the anatomical size differences between murine and human microvasculature, whereby Loa mf are hindered when traversing murine capillary beds. Alternatively, or in addition, because Loa exhibits a diurnal periodicity in humans42, physiological cues for oscillatory peripheral circulatory migration versus cardiopulmonary sequestration may vary between mice and humans. Similarly, human sub-period strain B. malayi also demonstrate a tropism for cardiopulmonary circulation when infused into mice21,24. Adult splenectomy of WT mice improved parasitaemia yields yet SCID mice (without splenectomies) supported the highest parasitaemias and splenectomies of SCID mice did not further elevate microfilaraemias. This suggests that any splenic mediated clearance of mf is part of an adaptive immune-dependent process.

Consequently, we were able to validate that rapid microfilaricidal activity of IVM against blood-borne Loa mf could be modelled in both immunodeficient and -competent mouse strains and subsequently explored the dependence of adaptive immune processes in IVM-mediated microfilaricidal efficacy. Our data demonstrate that typical, rapid, >90% clearance of mf from both cardiopulmonary and peripheral blood by either oral or parenteral, single dose IVM does not require adaptive immunity. This was in marked contrast to a lack of in vitro activity of IVM or the related, more potent macrocyclic lactone, moxidectin, at physiologically relevant exposures of drug. However, we determined that antigen-experienced, immunocompetent mice were subtly more sensitive to the effects of IVM clearance of Loa mf. Our data are consistent with previous findings that IVM can mediate high microfilaricidal activities against Brugia or Onchocerca mf in lymphopenic mouse strains21,24,43, and we conclude that whilst adaptive immunity is not a necessary host-directed component of the IVM microfilaricidal mode of action, variation in adaptive immune potential may influence magnitude of treatment response post-IVM treatment of loaisis individuals. Because we have previously developed, validated and implemented a CB.17 SCID mouse model to test macrofilaricidal activities against Brugia and Onchocerca adult filariae21,22,23,24,25, the CB.17 SCID Loa microfilaraemic mouse model is ideal to be implemented as a corresponding counter-screen to scrutinise for ‘off-target’ rapid, direct microfilaricidal activities. By using the same inbred strain, significant discrepancies in drug exposures between macrofilaricide and microfilaricidal efficacy tests should be avoided. We initially implemented the screen to test for ‘off-target’ activities of a veterinary anthelmintic, oxfendazole, which has undergone phase I trials as a repurposed treatment for human helminthiases ( NCT03035760) or the oral reformulation of flubendazole and determined that both benzimidazole anthelmintic chemotypes have no rapid IVM-like activity at dosages known to mediate macrofilaridal activity in preclinical mouse models24,29.

Beyond the immediate translational research priorities of new drugs and diagnostics for filarial diseases in loiasis co-morbidities, the aetiology of loiasis adverse reactions needs to be more thoroughly understood. Determining the pathophysiology of Loa AE is critical if effective adjunct therapies are to be deployed during IVM administration to at-risk groups to reduce the risk of AE and increase population adherence to MDA. Adjunct therapy is foreseeable as part of a ‘test-and-not-treat’ strategy using the recently developed Loa CellScope point-of-care device that can discern low-moderate, high or very high microfilaraemias, as a traffic light-warning system44,45. We therefore exploited the susceptibility of WT mice to Loa microfilaraemias post-immune priming to initially explore the systemic inflammatory responses induced by rapid IVM-mediated clearance of mf from the blood. We chose to examine these responses in ‘antigen experienced’ animals to more align with chronically infected human populations. Whilst initially both type-1 (IFNγ) type-2 (IL-4, IL-5, CCL11) and regulatory type (IL-10) inflammatory mediators were upregulated post-IVM treatment, by 7 days a switch to a predominant type-2 inflammatory signature was apparent, characterised by maintenance of IL-4 and IL-5, downregulation of IFNγ and IL-10 and significant increases of the eosinophil chemotactic factor CCL11. We have further characterised an augmented eosinophilia in peripheral circulation, in secondary lymphoid tissue and in the peritoneal cavity of antigen experienced, microfilaraemic mice as a consequence of IVM treatment. This suggests a predominance of allergic immune responses are induced post IVM, probably induced by liberation of mf somatic antigens, which may be targetable via anti-allergy/asthma type therapeutics. Certainly, eosinophil-containing micro-lesions have been identified in brain capillaries post-IVM treatment of baboons19 and both increased IL-5 and eosinophilia is evident in loiasis patients post-IVM or DEC treatment46 corroborating that eosinophilic responses in the research model emulate clinical inflammation post treatment. Considering the availability of a full spectrum of murine biological research reagents and transgenic animals, the research model now offers a powerful new approach to dissect inflammatory AE, acute tissue pathologies and evaluate therapeutic targeting of host inflammation post-IVM treatment.

Current limitations of both research models include the proximity to a source of Loa L3, necessary continued usage of experimentally infected baboons to provide mf and restraints on the numbers of L3 that can be acquired via trapping of wild flies. This means that loiasis mouse models are not currently available outside of the endemic region of Central Africa. However, we are investigating approaches to experimentally infect Chrysops with purified mf to increase throughput of infectious stage larvae. Preliminary ongoing experiments support that microinjections of L. loa mf into wild-caught Chrysops can yield infectious stage larvae, which develop into juvenile adult worms in mice. Following ethical permissions, we intend to evaluate whether purifications of mf from hypermicrofilaraemic human donors can be used to obviate the requirements for NHP experimentation and further increase throughput. Such experiments may also define the extent of diurnal periodic migrations displayed by blood-borne mf within microfilaraemic mouse models. Certainly, preliminary studies in splenectomised baboons indicate diurnal fluctuations of human strain L. loa are apparent. Further, we are validating whether using cryopreservations of mf or L3 can extend the accessibility of the models to non-endemic country research laboratories. Another present limitation of the infusion model to study treatment-associated pathology is that overt neurological-type AE has not yet been observed post-IVM delivery. However, we are currently investigating the fate of mf post treatment, including tropism and histopathological consequences in brain-associated vasculature, and whether increasing inoculates of mf in SCID or WT mice will lead to evidence of neurological dysfunction post treatment.

For basic biology research of loiasis and other filariae, establishing mouse models will be a powerful new tool to interrogate important host–parasitological interactions, such as how periodicity is influenced by host factors and dissecting stage-specific immune responses to larvae, adults and mf. Similarly, by establishing microinjections of mf derived from mice into Chrysops vectors, detailed, timed infection-courses could reveal new biological insights of the parasite–vector biology.

In conclusion, we have developed novel small animal models of loiasis sufficiently robust for immediate implementation in preclinical research to accelerate development of novel drugs, therapeutics and diagnostics for filariasis elimination in Central Africa.



BALB/c, BALB/c RAG2−/−γc−/−, CB.17 SCID, NOD.SCID and NOD.SCIDγc−/− (NSG) mice of 5–6 weeks of age were purchased from Charles River Europe, and BALB/c RAG2−/− mice were kindly provided by Prof Andrew McKenzie (MRC Laboratory of Molecular Biology, Cambridge University, UK) and by Prof. Dr. Antonius Rolink (Developmental and Molecular Immunology Department of Biomedicine, University of Basel, Switzerland). Mice were shipped in filter topped boxes to Research Foundation for Tropical Diseases and the Environment (REFOTDE), Buea, Cameroon. All mice were reared in REFOTDE in a 12:12 light:dark cycle, maintained in individually ventilated caging (IVC) with HEPA filtered air system (Tecniplast) with ad libitum provision of standard irradiated rodent chow and bottled mineral water. All mice used for the experiments were infected in the laboratory of REFOTDE. All animal procedures received ethical approval by the Animal Care Committee at REFOTDE and undertaken in accordance with UK regulatory standards.

L. loa microfilariae (mf) were obtained from splenectomised infected baboons (Papio anubis) that were kept in captivity and infected with the L. loa human strain17,32,47. The acquisition, care and ethical concerns on the use of baboons as donors of mf have been previously documented18,20. Ethical and administrative approvals for the use of baboons in this study were obtained from the Ministry of Scientific Research and Innovation of Cameroon (Research permit #028/MINRESI/B00/C00/C10/C12) and the Animal Care Committee at REFOTDE. Procedures adhered to the NIH Guide for the Care and Use of Laboratory Animals. The authors have complied with all relevant ethical regulations for animal testing and research.


L. loa mf were extracted from the blood using a Percoll® gradient centrifugation processing18,32,48 with a discontinuous gradient of 65%, 50% and 40% iso-osmotic Percoll®. Two milliliter of whole blood collected on the same day were loaded on the top of the gradient and centrifuged at 400 g for 20 min; the layer containing mf was carefully removed and filtered gently through a 5- µm pore-size cellulose filter, and mf were then transferred into a Petri dish containing the culture medium (10% foetal calf serum (FCS) supplemented Dulbecco’s modified Eagle’s medium (DMEM) and incubated 5 min/37 °C to release mf. Suspensions were then centrifuged to concentrate mf. Unless stated otherwise, 4 × 104 mf in 150 µl of RPMI were loaded in 26 G 1 -ml insulin syringes and maintained at 37 °C until intravenously injected in the tail vein of the mice.

L. loa L3 infective stages were derived from wild-caught Chrysops silacea via baited traps in a known hyperendemic area. Flies were dissected to allow release of any L. loa L3 infective stages. Infective doses of 100–200 L3 per 200 µL of medium (DMEM + 10% FCS) were loaded in 25 G 1 -mL syringes and subcutaneously injected into mice.

L. Loa adult worms were obtained from CB.17 SCID, NOD.SCID, NOD.SCIDγc−/− (NSG) and BALB/c RAG2−/−γc−/− mice that were infected with L. loa L3 and culled either at 3 or 5 months post infection. Worms were then either subcutaneously re-implanted into new recipient mice, fixed for histology or utilised in embryogram assays.

Experimental infections and drug treatments

Mice were infected with either 100 or 200 L.loa L3 via subcutaneous injection or with 5 male/5 female L. loa adult worms via surgical subcutaneous implantation or 4 × 104L. loa mf via a tail vein infusion. In the case of surgical implantation, mice were placed under anaesthesia using intra-peritoneal injections of ketamine (Ketaset, 70 mg/kg) and medetomidine (Domitor, 0.8 mg/kg) with surgery, post-operative monitoring and recovery21. L. loa adults were washed in several changes of the medium (DMEM + 10% FCS), and groups of five females and five males were surgically implanted under the dorsal back skin behind the neck.

For immune priming experiments, aliquots of 3 × 104 L. loa mf were killed through three cycles of 10 min at + 50 °C followed by 10 min at −50 °C incubations. Aliquots of 3 × 104 dead L. loa mf were subcutaneously injected to each mouse. Mice were challenged with 4 × 104L. loa mf 14 days post-immune priming.

Mice were treated orally with ivermectin (Sigma-Aldrich) at 1 mg/kg in water, with ivermectin subcutaneous injections at 5 mg/kg in water, orally with flubendazole (Janssen BEND formulation, a gift from Dr B. Baeton, Jansssen Pharmaceutica, Beerse, Belgium) at 40 mg/kg24,29, or orally with oxfendazole (Dolthene formulation, Vetsend) at 25 mg/kg in corn oil.

Mice were euthanized using CO2 rising concentrations. Post-mortem, blood was collected by cardiac puncture using either a heparinized 25 G needle and 1 -mL syringe for plasma collection or a non-heparinized syringe and needle for thick smears and serum collection followed by systematic dissection for adult parasite recovery.

Peripheral and cardiopulmonary microfilaraemias

Infected mice were checked for the presence of mf in blood by thick smear and subsequent Giemsa staining. Briefly, blood was collected from the tail vein (2 × 20 µL) or from the heart (2 × 50 µL) at necropsy using a 25 G 1 -mL syringe, transferred onto glass slides and then processed for thick smears through a scratch method. Air-dried smears were incubated in distilled water for 4 min to lyse erythrocytes, fixed in methanol for 1 min and finally stained with 40% Giemsa for 40 min then washed in distilled water until clear. Duplicate slides were counted twice with microscope operators blinded to treatment group.

Serological studies

Mouse sera or plasma were tested for filarial antigen detection using two kits commercially available for the detection of Wuchereria bancrofti antigens: the filariasis test strip (FTS, Alere, Abbott, UK) and the Og4C3 filariasis antigen ELISA (Tropbio, Cellabs, UK), both as per the manufacturer’s instructions. A volume of 70 μLof fresh serum was used immunochromatographic detection with the FTS per test strip with reading taken within minutes after sample application.

Plasma cytokines/chemokines levels in mouse plasma were determined using a 32-analyte multiplex cytokine immunoassay based on xMAP technology (MCYTMAG-70K-PX32 kit, Millipore) as per the manufacturer’s instructions and samples were analysed on a LX100TM multiplexing instrument (Luminex). Analytes included were: eotaxin, G-CSF, GM-CSF, M-CSF, gamma interferon (IFN-γ), TNF-α, IL-1α, IL-1β, IL-2, IL-3, IL-4, IL-5, IL-6, IL-7, IL-9, IL-10, IL-12 (p40), IL-12 (p70), IL-13, IL-15, IL-17, IP-10, CCL2, CCL3, CCL4, CCL5, CXCL1, CXCL2, CXCL5, CXCL9, leukaemia inhibitory factor (LIF) and vascular endothelial growth factor (VEGF).

Flow cytometry

Mouse peritoneal cells were collected via a peritoneal cavity wash with 10 mL of PBS-5% FCS. Single-cell suspensions were prepared in FACS buffer (PBS + 0.5% BSA + 2 mM EDTA). Fc receptors were blocked with αCD16/32 (1/40 dilution, ref: 14-0161-82, eBioscience) prior to the application of the following cocktail: viability dye eFluor450 (ref: 65-0863-14, eBioscience), anti-mouse SiglecF-APC (dilution 1/40, clone S17007L, ref: 155508, Biolegend) and anti-mouse Ly6G-FITC (dilution 1/40, clone RB6-8C5, ref: 11-5931-82, eBioscience) or their matched isotype controls using a fluorescence-minus-one method. Samples were fixed in FACS buffer containing 0.5% PFA and shipped at 4 °C to UK. All multi-labelled cell samples were subsequently acquired using a BD LSR II flow cytometer (BD Bioscience) and analysed on FlowJo Software (Supplementary Fig. 7). OneComp eBeads (eBioscience) were used to optimise antibody staining panels and apply compensation. For compensation controls, optimal PMT voltages for the positive signal to be detected were set within 104 and 105 whereas negative signal was set to below 102.

Differential blood count thin smears

Thin smears were performed on peripheral blood collected from the mouse tail vein and were stained in May–Grünwald (Sigma) for 5 min then in 40% Giemsa for 30 min. Leucocytes numeration was performed under a microscope counting 200 leucocytes. Operators were blinded to mouse groups.

Histological studies

Female and male worms were processed as whole mounts for anatomical observation. Worms were fixed in hot 70% ethanol then mounted on a glass slide within drops of glycerol. Samples were allowed an overnight incubation a room temperature to fully perfuse the worms with glycerol, and worms were analysed on an Olympus BX60 microscope.

Spleens from mice were collected at readout and fixed in 10% PFA for 24 h then transferred in 70% ethanol and subsequently embedded in paraffin. Paraffin sections (5 μm) were stained with hematoxylin-eosin (H&E, VWR) for the detection of eosinophils. Images were acquired using the digital slide scanner HPF-NanoZoomer RS2.0 (Hamamatsu) coupled to a high definition 3-CCD digital camera of the PHIC immunohistochemistry platform (Institut Paris-Saclay d’Innovation Thérapeutique, France). Eosinophils were counted from 10 quadrants of 120 µm x 200 µm per splenic zone per mouse. Operator was blinded to mouse group.

Statistical analysis

Data were first checked for normality, using D’Agostino & Pearson omnibus Shapiro–Wilk normality tests before or post log10 transformation of raw data. If raw or transformed data passed both tests, two-tailed parametric Student’s T -Test (two variables) or one-way ANOVA with Dunnett’s post-hoc tests (> two variables) were used. If the data failed to pass normality testing, two-tailed Mann–Whitney (two groups) or Kruskal–Wallis with Dunn’s post-hoc tests (>two variables) were used. Significant changes in paired data were tested by T tests or Wilcoxon tests. All tests were performed in GraphPad Prism software at a significance level of 5% and significance is indicated: *p < 0.05, **p < 0.01, ***p < 0.001. Heatmap analysis was undertaken in Excel using conditional formatting with −10-fold change being colour-coded as blue and +10 fold change being reported as red.

Reporting summary

Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The data that support the findings of this study are available from the corresponding author upon reasonable request.

Additional information

Journal peer review information: Nature Communications thanks David Abraham and the other anonymous reviewers for their contribution to the peer review of this work. Peer reviewer reports are available.

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.


  1. 1.

    Metzger, W. G. & Mordmuller, B. Loa loa-does it deserve to be neglected? Lancet Infect. Dis. 14, 353–357 (2014).

  2. 2.

    Zoure, H. G. et al. The geographic distribution of Loa loa in Africa: results of large-scale implementation of the Rapid Assessment Procedure for Loiasis (RAPLOA). PLoS. Negl. Trop. Dis. 5, e1210 (2011).

  3. 3.

    Boussinesq, M. Loiasis. Ann. Trop. Med. Parasitol. 100, 715–731 (2006).

  4. 4.

    Carme, B., Mamboueni, J. P., Copin, N. & Noireau, F. Clinical and biological study of Loa loa filariasis in Congolese. Am. J. Trop. Med. Hyg. 41, 331–337 (1989).

  5. 5.

    Noireau, F., Apembet, J. D., Nzoulani, A. & Carme, B. Clinical manifestations of loiasis in an endemic area in the Congo. Trop. Med. Parasitol. 41, 37–39 (1990).

  6. 6.

    Pinder, M. Loa loa - a neglected filaria. Parasitol. Today 4, 279–284 (1988).

  7. 7.

    Chesnais, C. B., Takougang, I., Paguele, M., Pion, S. D. & Boussinesq, M. Excess mortality associated with loiasis: a retrospective population-based cohort study. Lancet Infect. Dis. 17, 108–116 (2017).

  8. 8.

    Gardon, J. et al. Serious reactions after mass treatment of onchocerciasis with ivermectin in an area endemic for Loa loa infection. Lancet 350, 18–22 (1997).

  9. 9.

    Ducorps, M. et al. [Secondary effects of the treatment of hypermicrofilaremic loiasis using ivermectin]. Bull. Soc. Pathol. Exot. 88, 105–112 (1995).

  10. 10.

    Bockarie, M. J., Kelly-Hope, L. A., Rebollo, M. & Molyneux, D. H. Preventive chemotherapy as a strategy for elimination of neglected tropical parasitic diseases: endgame challenges. Philos. Trans. R. Soc. Lond. B. Biol. Sci. 368, 20120144 (2013).

  11. 11.

    Senyonjo, L. et al. Factors associated with ivermectin non-compliance and its potential role in sustaining onchocerca volvulus transmission in the west region of Cameroon. PLoS. Negl. Trop. Dis. 10, e0004905 (2016).

  12. 12.

    Basanez, M. G. et al. River blindness: mathematical models for control and elimination. Adv. Parasitol. 94, 247–341 (2016).

  13. 13.

    Kim, Y. E. et al. Control, elimination, and eradication of river blindness: scenarios, timelines, and ivermectin treatment needs in Africa. PLoS. Negl. Trop. Dis. 9, e0003664 (2015).

  14. 14.

    Taylor, M. J., Hoerauf, A., Townson, S., Slatko, B. E. & Ward, S. A. Anti-Wolbachia drug discovery and development: safe macrofilaricides for onchocerciasis and lymphatic filariasis. Parasitology 141, 119–127 (2014).

  15. 15.

    Pion, S. D., Boussinesq, M. & Kamgno, J. Treating Onchocerciasis in Regions in Which Loa loa Is Endemic. New Engl. J. Med 378, 871 (2018).

  16. 16.

    Duke, B. O. L. Studies on loiasis in monkeys II. The population dynamics of the microfilariae of Loa in experimentally infected drills (Mandrillus leucophaeus). Ann. Trop. Med. Parasit. 54, 15–31 (1960).

  17. 17.

    Orihel, T. C. & Moore, P. J. Loa loa: experimental infection in two species of African primates. Am. J. Trop. Med. Hyg. 24, 606–609 (1975).

  18. 18.

    Wanji, S. et al. Parasitological, hematological and biochemical characteristics of a model of hyper-microfilariaemic Loiasis (Loa loa) in the Baboon (Papio anubis). PLoS. Negl. Trop. Dis. 9, e0004202 (2015).

  19. 19.

    Wanji, S. et al. Ivermectin treatment of Loa loa hyper-microfilaraemic baboons (Papio anubis): assessment of microfilarial load reduction, haematological and biochemical parameters and histopathological changes following treatment. PLoS. Negl. Trop. Dis. 11, e0005576 (2017).

  20. 20.

    Tendongfor, N. et al. The human parasite Loa loa in cytokine and cytokine receptor gene knock out BALB/c mice: survival, development and localization. Parasit. Vectors 5, 43 (2012).

  21. 21.

    Halliday, A. et al. A murine macrofilaricide pre-clinical screening model for onchocerciasis and lymphatic filariasis. Parasit. Vectors 7, 472 (2014).

  22. 22.

    Aljayyoussi, G. et al. Short-course, high-dose rifampicin achieves Wolbachia depletion predictive of curative outcomes in preclinical models of lymphatic filariasis and onchocerciasis. Sci. Rep. 7, 210 (2017).

  23. 23.

    Turner, J. D. et al. Albendazole and antibiotics synergize to deliver short-course anti-Wolbachia curative treatments in preclinical models of filariasis. Proc. Natl. Acad. Sci. USA 114, E9712–E9721 (2017).

  24. 24.

    Sjoberg, H. et al. Short-course, oral flubendazole does not mediate significant efficacy against Onchocerca adult male worms or Brugia microfilariae in murine infection models. PLoS. Negl. Trop. Dis. 13, e0006356 (2019).

  25. 25.

    Sharma, R. et al. Minocycline as a re-purposed anti-Wolbachia macrofilaricide: superiority compared with doxycycline regimens in a murine infection model of human lymphatic filariasis. Sci. Rep. 6, 23458 (2016).

  26. 26.

    Turner, J. D. et al. Interleukin-4 activated macrophages mediate immunity to filarial helminth infection by sustaining CCR3-dependent eosinophilia. PLoS. Pathog. 14, e1006949 (2018).

  27. 27.

    Pion, S. D. et al. Positivity of antigen tests used for diagnosis of lymphatic filariasis in individuals without Wuchereria bancrofti Infection but with high Loa loa microfilaremia. Am. J. Trop. Med. Hyg. 95, 1417–1423 (2016).

  28. 28.

    Wanji, S. et al. Further evidence of the cross-reactivity of the Binax NOW(R) Filariasis ICT cards to non-Wuchereria bancrofti filariae: experimental studies with Loa loa and Onchocerca ochengi. Parasit. Vectors 9, 267 (2016).

  29. 29.

    Hübner, M. P. et al. Macrofilaricidal efficacy of single and repeated oral and subcutaneous doses of flubendazole in Litomosoides sigmodontis infected jirds. PLoS. Negl. Trop. Dis. 13, e0006320 (2019).

  30. 30.

    Geary, T. G. & Mackenzie, C. D. Progress and challenges in the discovery of macrofilaricidal drugs. Expert. Rev. Anti. Infect. Ther. 9, 681–695 (2011).

  31. 31.

    Zofou, D. et al. Evaluation of in vitro culture systems for the maintenance of microfilariae and infective larvae of Loa loa. Parasit. Vectors 11, 275 (2018).

  32. 32.

    Njouendou, A. J. et al. Heterogeneity in the in vitro susceptibility of Loa loa microfilariae to drugs commonly used in parasitological infections. Parasit. Vectors 11, 223 (2018).

  33. 33.

    Moreno, Y., Nabhan, J. F., Solomon, J., Mackenzie, C. D. & Geary, T. G. Ivermectin disrupts the function of the excretory-secretory apparatus in microfilariae of Brugia malayi. Proc. Natl. Acad. Sci. USA 107, 20120–20125 (2010).

  34. 34.

    Maizels, R. M. & Denham, D. A. Diethylcarbamazine (DEC): immunopharmacological interactions of an anti-filarial drug. Parasitol 105, S49–S60 (1992).

  35. 35.

    Spolski, R., Gromer, D. & Leonard, W. J. The γ (c) family of cytokines: fine-tuning signals from IL-2 and IL-21 in the regulation of the immune response. F1000Res. 6, 1872 (2017).

  36. 36.

    Vivier, E. et al. Innate Lymphoid Cells: 10 Years On. Cell 174, 1054–1066 (2018).

  37. 37.

    Boyd, A., Killoran, K., Mitre, E. & Nutman, T. B. Pleural cavity type 2 innate lymphoid cells precede Th2 expansion in murine Litomosoides sigmodontis infection. Exp. Parasitol. 159, 118–126 (2015).

  38. 38.

    Patton, J. B. et al. Methylprednisolone acetate induces, and Δ7-dafachronic acid suppresses, <em>Strongyloides stercoralis</em> hyperinfection in NSG mice. Proc. Natl. Acad. Sci. 115, 204 (2018).

  39. 39.

    Korten, S. et al. Expansion of NK cells with reduction of their inhibitory Ly-49A, Ly-49C, and Ly-49G2 receptor-expressing subsets in a murine helminth infection: contribution to parasite control. J. Immunol. 168, 5199 (2002).

  40. 40.

    Globisch, D. et al. Validation of onchocerciasis biomarker N-acetyltyramine-O-glucuronide (NATOG). Bioorg. & Med. Chem. Lett. 27, 3436–3440 (2017).

  41. 41.

    Lagatie, O. et al. Evaluation of the diagnostic potential of urinary N-Acetyltyramine-O,β-glucuronide (NATOG) as diagnostic biomarker for Onchocerca volvulus infection. Parasit. Vectors 9, 302 (2016).

  42. 42.

    Hawking, F. Periodicity of microfilariae of Loa loa. Trans. R. Soc. Trop. Med. Hyg. 49, 132–142 (1955).

  43. 43.

    Folkard, S. G., Taylor, M. J., Butcher, G. A. & Bianco, A. E. Protective responses against skin-dwelling microfilariae of Onchocerca lienalis in severe combined immunodeficient mice. Infect. Immun. 65, 2846–2851 (1997).

  44. 44.

    D’Ambrosio, M. V. et al. Point-of-care quantification of blood-borne filarial parasites with a mobile phone microscope. Sci. Transl. Med 7, 286re284 (2015).

  45. 45.

    Kamgno, J. et al. A test-and-not-treat strategy for onchocerciasis in Loa loa-endemic areas. N. Engl. J. Med. 377, 2044–2052 (2017).

  46. 46.

    Herrick, J. A. et al. Posttreatment reactions after single-dose diethylcarbamazine or ivermectin in subjects with Loa loa infection. Clin. Infect. Dis. 64, 1017–1025 (2017).

  47. 47.

    Wanji, S., Tendongfor, N., Vuong, P. N., Enyong, P. & Bain, O. The migration and localization of Loa loa infective and fourth stage larvae in normal and immuno-suppressed rodents, consequences in human pathology. Ann. Trop. Med. Parasit. 96, 823–840 (2002).

  48. 48.

    Van Hoegaerden, M., Fau - Ivanoff, B. & Ivanoff, B. A rapid, simple method for isolation of viable microfilariae. Am. J. Trop. Med. Hyg. 35, 148–151 (1986).

Download references


The authors would like to thank Benny Baeton and Marc Englen (Janssen Pharmaceutica, Beerse) for the donation of oral flubendazole formulation, Dr Marc Hubner (University Clinic Bonn) for helpful advice on oxfendazole oral dosing, Prof. Andrew McKenzie (MRC Laboratory of Molecular Biology, Cambridge University, United Kingdom) and Prof. Dr. Antonius Rolink (Developmental and Molecular Immunology Department of Biomedicine, University of Basel, Switzerland) for providing BALB/c RAG2−/− mice and Oben Bruno for husbandry of experimental baboons. We also thank Francoise Gaudin and the PHIC immunohistochemistry platform (Institut Paris-Saclay d’Innovation Thérapeutique, France). This work was supported by a Bill and Melinda Gates Foundation Grand Challenges Explorations Grant (OPP1119043) to J.D.T., S.W. and M.J.T.

Author information

Conceptualisation: J.D.T., S.W. and M.J.T. Methodology: J.D.T., S.W., N.P.P. and H.S. Formal analysis: J.D.T., S.W., N.P.P., H.S., H.M.M. and V.C.C. Resources: J.D.T. and S.W. Writing: N.P., J.D.T., H.S. and S.W. Investigation: N.P., H.S., H.M.M., V.C.C., A.J.N., F.F.F., D.B.T., N.V.G., D.N.A., P.W.C., B.L.N., S.W. and J.D.T. Funding acquisition: J.D.T., S.W. and M.J.T.

Competing interests

The authors declare no competing interests.

Correspondence to Joseph D. Turner.

Supplementary information

Supplementary Information

Peer Review File

Reporting Summary

Description of Additional Supplementary Files

Supplementary Movie 1

Supplementary Movie 2

Supplementary Movie 3

Supplementary Movie 4

Rights and permissions

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

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.