Malaria liver stages represent an ideal therapeutic target with a bottleneck in parasite load and reduced clinical symptoms; however, current in vitro pre-erythrocytic (PE) models for Plasmodium vivax and P. falciparum lack the efficiency necessary for rapid identification and effective evaluation of new vaccines and drugs, especially targeting late liver-stage development and hypnozoites. Herein we report the development of a 384-well plate culture system using commercially available materials, including cryopreserved primary human hepatocytes. Hepatocyte physiology is maintained for at least 30 days and supports development of P. vivax hypnozoites and complete maturation of P. vivax and P. falciparum schizonts. Our multimodal analysis in antimalarial therapeutic research identifies important PE inhibition mechanisms: immune antibodies against sporozoite surface proteins functionally inhibit liver stage development and ion homeostasis is essential for schizont and hypnozoite viability. This model can be implemented in laboratories in disease-endemic areas to accelerate vaccine and drug discovery research.
Malaria is a major global disease with almost half of the world’s population at risk, resulting in an estimated 216 million cases and 445,000 deaths in 20161. The two most prevalent causes of malaria are apicomplexan parasites P. falciparum, the most virulent and dominant species in Sub-Saharan Africa, and P. vivax, with the widest geographical distribution and major economic impact2,3,4. Plasmodium sporozoites initiate infections when injected into the dermis by a female anopheline mosquito and then use a molecular motor-driven mechanism to rapidly enter the human circulatory system and translocate across the liver sinusoid5,6,7. After invasion of hepatocytes, liver-resident parasites undergo asexual schizogony to form tens of thousands of merozoites. Following merozoite egress from the infected liver cell, the parasites escape into the hepatic vein to infect erythrocytes where they asexually replicate in circulation, leading to geometric population expansion and the clinical symptoms of malaria. Although it is the blood-stage infection that causes clinical disease, the sporozoite and the liver stage (LS) forms, which together are referred to as pre-erythrocytic (PE) stages, represent a vulnerable bottleneck for therapeutic interventions to prevent malaria8,9. Therefore, chemotherapeutic and immunoprophylactic interventions have converged on targeting P. vivax and P. falciparum PE stages as a strategy to block progression to clinical malaria and transmission10.
The biology of the P. vivax and P. falciparum LS forms fundamentally differ as some P. vivax parasites will remain quiescent as uninucleate stages termed hypnozoites11. Hypnozoites are not susceptible to the mechanism of action of most antimalarial drugs and can persist for weeks, months, or even years before an unknown re-activation mechanism stimulates completion of development and a symptomatic blood-stage infection12. In addition, P. vivax is able to rapidly form transmissible gametocytes in circulation before presentation of clinical symptoms13. Therefore, an effective malaria elimination toolbox has been proposed consisting of a multi-stage drug with hypnozonticidal activity and a highly efficacious vaccine conferring life-long sterile immunity; however, neither of these tools is currently available10. Malaria control is now focused on treating the symptomatic blood and transmission stages with front-line drugs of Artemisinin Combination Therapies (ACTs) for falciparum malaria and predominately chloroquine (CQ) for vivax malaria1,14. Prophylactic regimens of atovaquone and proguanil (Malarone®) target only the LS schizont, while the only chemotherapeutic intervention currently capable of targeting hypnozoites are 8-aminoquinolines, such as primaquine and tafenoquine15,16. Unfortunately, use of 8-aminoquinolones is contraindicated in many malaria endemic countries because of its toxicity in individuals with some glucose-6-phosphate dehydrogenase (G6PD) polymorphisms, restricting mass drug administration campaigns in regions where high-risk favisms are common17. In regards to malaria vaccinology, development of PE vaccines has focused on the initial stages of infection targeting antibodies to the sporozoite surface to neutralize parasite migration to the liver and consequently the disease-causing blood stage18,19,20. However, vaccines to prevent malaria have lagged far behind drug development efforts as only one vaccine for P. falciparum has been licensed, RTS,S-S/ASO1 or MosquirixTM21. In Phase III clinical field trials MosquirixTM showed a temporary, age-specific response with only partial protection22. Meanwhile, vaccines for P. vivax remain mostly in the pre-clinical discovery phase of development and only a few candidates have progressed into initial clinical trials23.
In vitro PE assays are essential for preclinical assessment of novel vaccines and drugs, yet currently available PE assays are inadequate for meeting the demands of a genuine PE screening effort24. Historically, many studies of Plasmodium liver models used human hepatoma lines, which are deficient in specific surface receptors present on primary human hepatocytes (PHHs) that are required for Plasmodium sporozoite invasion, resulting in poor invasion rates25,26. Furthermore, LS formation within hepatoma cells is atypical compared to that noted in animal models as the schizonts are smaller and cannot be as easily distinguished from hypnozoites and persistent proliferation of these host cells hinders image-based analysis27. More recent studies have used fresh, cryopreserved PHHs, or human iPSC-derived hepatocyte-like cells in a 96-well plate co-culture model, yet LS development rates (LS parasites per sporozoite inoculum) remained low despite sporozoite infection loads 10-fold higher than what we report herein25,28,29,30. Animal models engrafted with PHHs offer excellent Plasmodium LS development but intrinsically high costs and low-throughput hinders the use of this model for drug discovery31,32.
In this report we describe a robust anti-PE therapeutic screen streamlined for P. vivax and P. falciparum using a PHH culture system comprised entirely of commercially available 384-well plates and cell culture reagents. Reducing to a 384-well microtiter format promotes key morphological and functional characteristics of native in situ hepatocytes and allows for high-resolution imaging, seamless image acquisition with faster imaging speed, and integration of automated high-content image analysis. Identification of optimal sporozoite isolation and hepatocyte culture methods resulted in highly reproducible formation of hundreds of LS parasites in each well of a 384-well plate, making the model ideal for P. vivax and P. falciparum PE bioassays. Implementation of our PHH culture system in laboratories located in and outside of malaria endemic areas demonstrates this novel PE model will help fill a critical technology gap hindering advancement of PE-active therapies and lay the foundation for next-generation malaria control and elimination.
Functional human hepatocytes in a commercial 384-well plate
We discovered that the small-scale collagen-treated surface area of particular commercially available 384-well plates coupled with our methodology provides a suitable microphysiological environment for long-term cultivation of PHHs (Fig. 1a, Supplementary Fig. 1a). The PHH donor lots PDC and NLX, used for the majority of studies described herein, were seeded at a density of 1.8 × 104 live cells per well to achieve attachment of ~1 × 104 cells per well. High-content imaging (HCI) of the cultured PHHs revealed individual cells in a confluent layer organized into lobule-like multicellular units. A rapid re-acquisition of primary cell characteristics occurred within two days, including visible transport of biliary metabolites and active mitochondria, and then remained stable for at least 30 days (Fig. 2a).
Functionality and metabolic activity of cultured PHHs were further characterized by several biometrics. Albumin production leveled at day 4 and remained stable thereafter with slight variation between 2 and 4 ng ml−1 for a duration of 30 days (Fig. 2b, Supplementary Fig. 1b). Furthermore, PHHs maintained a CYP3A4 response to Rifampicin between days 4 and 20 along with stable factor IX expression for 3 weeks (Supplementary Fig. 1c, d). Hepatobilary transport (active and inactive) of the bile canaliculi was measured by staining with CellTrackerTM Green CMFDA and quantified by image analysis. This biomarker passes into hepatocytes whereupon it is trapped as cell-impermeable glutathione methylfluorescein (GS-MF) that is subsequently actively transported into the bile canaliculi. Accumulation of this biliary metabolite can be used to quantify the functional activity of multi-drug resistance-associated protein 2 (MRP2) to serve as a surrogate indicator of hepatocyte polarization28,33 (Supplementary Fig. 2). Characterization of transport by PHH lot PDC showed a steady increase of active bile canaliculi network formation within the monolayer of lobule-like microstructures coupled with continued growth in bile canaliculi length reaching maximum lengths of 122.90 µm with a mean length of 19.33 ± 9.01 µm (±standard deviation) on day 21 compared to a maximum length of 19.19 µm with a mean length of 11.90 ± 2.35 µm on day 2 (n = 3, n′ = 3) (Fig. 2c, d). We assessed an additional biomarker of hepatocyte viability by characterizing the electrical potential between the interior and exterior of functioning mitochondria using cell-permeant dye tetramethylrhodamine (TMRM), which produces a bright signal within polarized mitochondria34,35. Measuring mean fluorescence intensity (MFI) of cytoplasmic stain and then comparing the daily time points indicated a 4-fold increase of mitochondrial activity from day 2 to 21 (Fig. 2e). Further image analysis revealed co-localization of high mitochondrial activity and bile canaliculi growth (Mander’s coefficients M1, M2 = 1 and tM1, tM2 ≥ 0.3–0.8) with highest correlation during early bile duct formation on day 2 (r = 0.72) (Supplementary Fig. 3a–c)36,37. Altogether the in vivo-like physiological and morphological indicators of this in vitro liver platform were expected to be highly supportive for experimental studies of the major human malaria parasites, P. vivax and P. falciparum.
Complete development of P. vivax and P. falciparum LS parasites
To evaluate our model’s suitability for experimental studies with human malaria parasites, we tested cryopreserved PHH donor lots from four companies and subjected each to an experimental matrix to include a range of seeding densities and sporozoite isolation methods. In our hands, three lots tested from Bioreclamation IVT (BIVT) supported higher P. vivax and P. falciparum LS parasite development rates than lots tested from other sources (Supplementary Fig. 4a, Supplementary Table 1). We therefore decided to screen an additional 13 BIVT PHH donor lots for both P. vivax and P. falciparum development relative to lot PDC and the terminally-differentiated HepaRG hepatocyte line (as a negative control for LS development). Four donors, lots H, J, P, and Q, were significantly higher in LS development rate relative to PDC (P < 0.0001 and P < 0.05, two-way ANOVA followed by Dunnett’s multiple comparisons) while two donors, lot F and N did not support P. falciparum or P. vivax LS parasite growth. We also discovered some donors, lots G, H, I, and P, appeared susceptible to only P. falciparum or P. vivax (Fig. 3a). Three PHH donors did not form a monolayer in the 384-well microplate.
Following characterization of Plasmodium spp. sporozoite infection rate, this expanded set of PHH donor lots were assessed for basal metabolic CYP activity (Supplementary Table 2, Supplementary Fig. 5) and hepatic functionality by measurement of bile canaliculi formation and mitochondrial activity over 14 days (Supplementary Table 3). Interestingly when measured over days 2–8, PHH donors found to have a stable mean TMRM intensity ( ≥ 3000 MFI), increase of cytoplasmic-stained cell area substantial active bile transport ( ≥ 30%), and a decrease of total hepatocytes appeared to support higher Plasmodium LS developmental rates. Furthermore, PHH donor lots with only a 2-fold increase in mean TMRM intensity and increased amount of inactive transport on day 8 ( ≥ 50%) had attenuated Plasmodium LS development with a reduction in mean LS schizont area. Lastly, the absence of LS parasite development was only observed in PHH donor lots with a decrease in active transport and minimal change in mean TMRM intensity from day 2 to 8 (Supplementary Table 3). After identification of suitable PHH donor lots, other microenvironmental factors that might influence sporozoite invasion and LS development were optimized. Hepatocyte seeding density and time between seed and sporozoite infection were identified as crucial variables; the highest P. vivax LS development rates resulted from a seeding density of 1.8 × 104 live PHHs yielding a monolayer of ~1.0 × 104 cells, followed by a delayed sporozoite infection until at least day 3 to allow for monolayer assembly (Supplementary Fig. 4b–d).
The P. vivax sporozoites produced from mosquitoes fed on clinically-isolated blood meals consistently yielded superior LS developmental rates (2–8.30%) compared to sporozoites from mosquito infections derived from in vitro-cultured P. falciparum NF54-WT (0.60–2%) and P. falciparum NF54-GFP (0.04–0.40%) following an inoculum of 5.0 × 103 sporozoites (Fig. 3b, f, g). Characterization of day 6 LS parasites revealed synchronized growth of P. falciparum with 75.95% of the parasites having a mean parasite area of 73.82 ± 6.52 µm2 (n = 3, n′ = 8) (Fig. 3c, f). Inversely, P. vivax day 6 parasites developed asynchronously as the schizont population had larger, irregular parasite area compared to P. falciparum (Fig. 3c, g) ranging from 31.65 ± 0.97 to 1270 ± 197.30 µm2 (n = 3, n′ = 26). By day 8, some P. falciparum LS schizonts successfully completed maturation and released infectious merozoites leading to further variability in LS quantification and size distribution (Supplementary Fig. 6). Furthermore, P. vivax LS schizonts continued to grow remarkably larger from day 6 and nearly doubled in area with 32.44% LS having a mean area of 2709 ± 333.20 µm2 (n = 3, n′ = 26) (Fig. 3d, g and Supplementary Table 4). Importantly, from days 6 to 8, P. vivax LS hypnozoites represented ~60% of the total LS parasites per well with a mean size of 34.55 ± 2.37 µm2 (n = 3, n′ = 26) (Fig. 3e).
Developing LS forms of P. vivax and P. falciparum were analyzed by HCI using a panel of Plasmodium antibodies targeting proteins expressed at different stages of maturity (Fig. 4a–c). The P. vivax hypnozoites and schizonts were distinguishable by size beginning on day 4 post-infection with distinct individual merozoites evident in mature day 8 schizonts. In addition to the small sizes, hypnozoites stained positively for Upregulated In Infectious Sporozoite-4 (UIS4), a parasitophorous vacuole membrane (PVM) protein as previously noted, but were negative for both PVM markers Exported Protein-1 (EXP-1) and Exported Protein-2 (EXP-2) which function in active export in developing LS schizonts (Fig. 4a)31,38,39. Notably, day 8 P. vivax LS schizonts showed an accumulation of EXP-2 protein in unknown vacuoles suggesting a role in degradation or sequestration (Fig. 4b). All multinucleated developing stages of P. vivax and P. falciparum were stained positively for Acyl Carrier Protein (ACP) and Glyceraldehyde-3-Phosphate Dehydrogenase (GAPDH), providing evidence of active fatty acid biosynthesis and glycolysis39. In addition, mature LS schizonts had high cytoplasmic expression of Macrophage Migration Inhibitory Factor (MIF) and Heat Shock Protein 70 (HSP70) confirming these parasites expressed proteins to modulate the human host (Fig. 4b, c)31. Mature hypnozoites stained negative for Merozoite Surface Protein 1 (MSP1) whereas day 8 LS schizonts showed MSP1 surface localization on segmenting merozoites (Fig. 4a). Day 5 P. falciparum LS schizonts were positive for both MSP1 and MSP2, even though the diffuse cytoplasmic localization indicated merozoite segmentation was in process (Fig. 4c)40,41. Interestingly, a portion of P. vivax late-stage schizonts stained positive for Pvs16, a gametocyte-specific protein, suggesting some LS merozoites are pre-committed as first generation gametocytes prior to the erythrocytic cycle (Fig. 4d and Supplementary Fig. 7). Finally, to confirm complete LS parasite maturation in the 384-well PHH culture system, merozoite infectivity was evaluated by addition or overlays of highly enriched human CD 71+ reticulocytes to P. vivax LS cultures (days 9–11) and fresh human red blood cells (RBCs) to P. falciparum cultures (days 7–8). Within first 24 h of P. vivax overlays, merozoite packages (merosomes) were seen released into the collected media along with P. vivax-infected reticulocytes and although we did not attempt to observe P. falciparum merosomes, early ring-infected RBCs were detected and continued development within RBCs was observed (Fig. 4e).
Design consideration for treatment mode and HCI endpoint
Ideally, a P. vivax and P. falciparum PE therapeutic screening platform should capture anti-parasite inhibitory activity against sporozoite migration, hepatocyte infection, LS development, and blood-stage breakthrough. To achieve these objectives, assay designs were considered either prophylactic, to prevent infections, or radical cure, to eliminate existing infections (Fig. 1b). For evaluating prophylactic efficacy of vaccines, sporozoites were exposed to immune antibodies or sera at the time of or just prior to their addition to the hepatocyte cultures. Similarly, prophylactic drugs were evaluated for activity by exposure at the time of sporozoite infection. However, LS assays for P. vivax require evaluation for radical cure activity to eliminate mature hypnozoites, as early drug application (prior to day 4–5 post-infection) can be effective on immature hypnozoites but inactive on mature hypnozoites (day 5 and beyond)42. Regardless of treatment mode, all cultures were fixed prior to release of mature merozoites to enable HCI-based quantification of growth using our experimentally defined LS phenotypes based on size and differential protein expression (UIS4 and GAPDH) (Table 1). In our 4-step HCI-based screening assays, antibody reagents were chosen for their staining patterns to facilitate automated quantification by defining the full LS form to enable measurement of growth area by automated morphometric analyses. Quantified populations were then normalized to controls and dose response curves fitted to generate half-maximal effective concentration (EC50) and inhibitory concentration (IC50) in Collaborative Drug Discovery (CDD) Vault or Graphpad Prism (Fig. 5). Automated imaging and quantification on an Operetta or ImageXpress was highly robust with 95–100% accuracy in identifying developing LS schizonts and hypnozoites when compared to conventional manual techniques (Table 2). Overall, automated HCI rapidly increased screening throughput allowing at least three 384-well plates to be analyzed within 24 h on an Operetta using wide field mode and 8 h on an ImageXpress spinning disc confocal imaging system.
Anti-CSP antibodies show species-specific inhibition
Next, our LS platform was validated for inhibition of liver stage developmental assays (ILSDA; Fig. 1b) by examining specificity and sensitivity of well-characterized monoclonal antibodies (mABs), anti-PfCSP mAB 2A10, anti-PvCSP mAB 2F2, and PvCSP mAB 2E10.E943,44,45,46,47. Several ILSDA protocol optimizations lead to improved experimental results. First, we discovered that sporozoites of both species exposed to mABs in phosphate buffered saline (PBS) adversely affected ILSDA outcomes by significantly decreasing sporozoite viability, hepatocyte infection rates, and increasing false positives; therefore, a buffered cell culture medium (RPMI or hepatocyte culture media) was used for incubation with mAB (Supplementary Fig. 8a, b)24,45,48,49,50. Second, having found sporozoite invasion rates were improved by allowing the sporozoite–hepatocyte interaction to persist for 24 h instead of the conventional 3-h interaction followed by a wash step, ILSDAs were performed by co-incubation of sporozoites, mAB, hepatocytes, and media overnight instead of the typical sporozoite pre-treatment with mAB. Third, anti-PvCSP mAB 2F2 exhibited a minimal difference in IC50 values for sporozoites exposed to the mAB for 20 min prior to addition to hepatocytes vs. co-incubation of mAB, sporozoites, and hepatocytes (Supplementary Fig. 8c). Finally, the assay endpoint was extended to day 6 or 8 in order to identify potential late-stage developmental phenotypes that are not easily evaluated with current LS platforms using hepatoma cells.
Our HCI analysis at 6 days post-infection confirmed that anti-PvCSP mAB 2F2 completely inhibited P. vivax sporozoite invasion and LS development at concentrations of 250 µg ml−1 with an IC50 of 4.60 µg ml−1 (n = 3, n′ = 2) (Fig. 6a). This inhibition was specific, as P. falciparum sporozoites exposed to anti-PvCSP mAB 2F2 resulted in normal P. falciparum LS development and P. vivax sporozoites exposed to anti-PfCSP mAB 2A10 resulted in normal P. vivax LS development. These results were expected as anti-P. falciparum and P. vivax sporozoite immunity (natural immunity or by immunization with irradiated sporozoites) is directed towards the dominant Bc epitopes of the central repeat regions of mammalian CSPs, which are the epitope targets of these anti-CSP mABs. Similar analysis of P. vivax sporozoite attenuation with anti-PvCSP mAB 2F2 revealed a novel discovery that P. vivax LS parasites were significantly reduced in size and had lower DNA content, indicating post hepatocyte-invasion antibody inhibition of LS development (Fig. 6b, c). Moreover, additional day 8 ILSDAs performed with cryopreserved P. vivax VK247-positive sporozoites and anti-2E10.E9 mAB (targeting CSP subtype VKS247) obtained a similar IC50 (2.85 µg ml−1) compared to ILSDAs with fresh P. vivax sporozoites, indicating a possible use of cryopreserved sporozoites for standardized screening (Supplementary Fig. 9)51,52. While further study is needed, these results show our platform is suitable for gaining a deeper understanding of the activity of anti-CSP antibodies as we identified and quantified inhibitory effects manifesting during and after hepatocyte invasion.
Similar species-specific concentration-dependent results were obtained for P. falciparum sporozoite infection and development in PHHs using anti-PfCSP mAB 2A10. Conversely, anti-PvCSP mAB 2F2 had no measurable effect on P. falciparum development at any concentration (Fig. 6d). The higher concentrations of anti-PfCSP mAB 2A10 of 80 and 40 µg ml−1 led to a 100% functional inhibition of parasite development with elevated reduction (>50% inhibition) in parasite development across all remaining concentrations, respectively (Fig. 6d). Similar to the P. vivax ILSDA, P. falciparum sporozoites exposed to lower concentrations of antibody (10 µg ml−1) permitted hepatocyte infection but resulted in late-stage LS developmental growth defects and delayed maturation (Fig. 6e, f). This consistently observed growth attenuation activity suggests that in addition to invasion inhibition, an anti-sporozoite antibody can attenuate intracellular LS development through an unknown mechanism.
To determine the utility of the ILSDA to experimentally evaluate functional immunogenicity of novel vaccines, P. vivax and P. falciparum sporozoites were treated with mouse immune sera samples (G2, G3, G6, and G7) raised against a self-assembling protein nanoparticle (SAPN) (FMP014/ALF, FMP014/ALFQ, FMP014V/ALF, and FMP014V/ALFQ, respectively)53. Samples G2 and G3 were derived from immunization with the FMP014 monomer containing PfCSP CD4+ and CD8+ epitopes, universal TH epitopes, portions of the α-TSR domain, and 6 repeats of the NANP motifs of the PfCSP with differing Army Liposomal Formulation (ALF) based adjuvants (ALF or ALQ)53. Samples G6 and G7 were derived by immunization with a SAPN assembled from an FMP014V monomer containing two copies of the PvCSP (VKS type 210) repeat region motif and the α-TSR domain of PfCSP53. Invasion and development of P. falciparum sporozoites were inhibited in a dose-dependent manner similar to the anti-CSP mAB (Fig. 6g) for all four serum samples with G2 exhibiting the strongest inhibitions for all dilutions and a growth phenotype at 1:16 dilution. Alternatively, sample G6 only moderately inhibited P. vivax sporozoites and G7 showed 100% inhibition at lowest dilutions with an IC50 at 1:8 dilution (n = 2, n′ = 2) (Fig. 6g). The pre-bleed serum control showed minimal inhibitory effect compared to the unexposed sporozoite control (Supplementary Fig. 8d). To overcome experimental bias, all percent inhibition calculations were standardized to the pre-bleed serum control48.
Compound library screen targeting LS parasites
Several compound collections were screened for activity against P. vivax LS parasites in our LS platform following the drug treatment modes described in Fig. 1. Compounds from the MMV portfolio were tested in eight-point dose response assays, including triplicate controls (KDU691 and atovaquone) in addition to 36 compounds per plate, with concentrations ranging from 10 µM to 5 nM represented in singleton wells. In every assay plate, potent activity of phosphatidylinositol 4-kinase inhibitor (PI4K) KDU691 was confirmed against all forms except hypnozoites treated in the radical cure mode and atovaquone activity only against schizonts treated in prophylactic mode (Fig. 7a). To demonstrate multispecies capability and cross-species comparisons, a small subset of 6 MMV compounds were evaluated in the eight-point dose response assay against P. falciparum LS schizonts (Fig.7b and Supplementary Table 5). Compounds were tested in duplicate in two independent experiments in prophylactic mode only, as P. falciparum does not produce hypnozoites and completes development prior to the radical cure treatment times. Comparison of EC50 values between P. vivax and P. falciparum revealed similar efficacies between atovaquone, DSM421, P218, and KAF156. Pyrimethamine showed a potent EC50 at 0.026 µM for P. falciparum and was confirmed inactive against P. vivax when assayed at a single concentration of 10 μM54,55.
Next, a set of 913 repurposed compounds from the Calibr Bioactive Library were tested at 10 µM single concentration in the radical cure treatment mode. Compounds with schizonticidal or hypnozonticidal activity were identified, including one compound, monensin, showing complete activity against both forms (Fig. 7c, Supplementary Table 6). Monensin activity was more potent and rapidly clearing compared to 8-aminoquinolines, primaquine, and tafenoquine, which were negative for activity after 3 days of treatment in all assay modes except primaquine against schizonts following prophylactic treatment (Fig. 7d). A radical cure dose-response assay was performed to confirm the ability of monensin to clear hypnozoites and was found to be effective with an EC50 of 398 nM (n = 2, n′ = 3). Using our prophylactic 8-point dose response assay, we explored the efficacy of three other ionophores: nigericin, salinomycin and lasalocid-A56,57. All ionophores were found to potently inhibit all P. vivax LS development. Because many ionophores are toxic to specific species, we compared PHH nuclei counts to better understand ionophore selectivity index (Fig. 7d and Supplementary Table 6)58. Nigericin, in particular, cleared the culture of all parasite forms at all doses tested (EC50 < 5 nM) while hepatic toxicity was only noted at much higher doses (>100 nM), demonstrating a selectivity index of over 20. A subset of compounds were assayed in three different PHH lots, NLX, PDC, and UBV to identify host-cell-specific effects on efficacy. Active compounds atovaquone and MMV390048, a PI4K inhibitor, were found similarly active across all donors, but prodrug primaquine was found active only in lots with higher CYP2D6 activity (Supplementary Table 2, Supplementary Fig. 10).
The lack of efficient high-throughput screening assays has been a major constraint limiting development of much needed new therapies targeting P. vivax and P. falciparum PE stages. The in vitro liver model reported here removes this barrier by significantly reducing the use of precious biological materials; each individual assay unit requires only 1.0 × 104 hepatocytes and only 5.0 × 103 P. vivax or P. falciparum sporozoites, representing a >20-fold reduction per assay unit relative to current platforms28,29,30,50. When extrapolated for a full 384-well plate run at least 2.0 × 106 sporozoites are required per plate, a practical number to obtain from dissection of salivary glands from 20 to 200 mosquitoes. Nonetheless, this small cell culture surface area of only 10 mm2 typically supported >200 P. vivax or >50 P. falciparum LS parasites per well, exceeding the averages of infected hepatocytes obtained in traditional models using larger 96-well plates59,60.
We attribute our improved sporozoite isolation and infection techniques, as well as access to properly cryopreserved hepatocytes as the key factors responsible for the greatly improved infection rates. Following characterization of 13 different PHH lots in addition to lot PDC and HepaRG, several lots from were found highly viable, monolayer-forming, and functional; all characteristics ideal for Plasmodium LS development (Supplementary Tables 2 and 3, Supplementary Fig. 5). However, the specificity of PHH lots for either P. falciparum or P. vivax may be better attributed to the hepatic phenotypes. Of all the PHH donor lots examined for sporozoite invasion and LS development, some lots were not supportive of either or both P. vivax and P. falciparum. We hypothesize this bimodal support of infection in otherwise healthy hepatocytes is a product of natural variation in presentation of hepatic surface receptors CD81 and SR-BI, as P. vivax and P. falciparum hepatocyte entry has been found receptor-specific61. While relative expression of surface receptors could not be analyzed in this study, additional proteomic and transcriptomic tools may be needed to identify biomarkers linked to a compatible donor phenotype. Alternatively, this variation could result from the cryopreservation process possibly leading to hepatocyte membrane receptor loss or undermining hepatic fitness to support intracellular parasites. Our hepatocyte bio-image assessment of the different PHH donor lots did suggest a strong link between enhanced sporozoite invasion and LS development to highly dynamic mitochondrial activity and increased bile canaliculi network formation. This indicates that the quality of hepatocyte lot may be more important than variation among individual donors. The mitochondria in hepatocytes are essential for survival, with main roles in energy metabolism (ATP), ion homeostasis, and apoptosis. Hepatic mitochondrial activity is likely vital in LS development, but host-parasite interactions are still largely uncharacterized and further investigation is needed62,63. Regardless, we demonstrate the advantage of using a pre-validated, effectively cryopreserved PHH lots over cell lines as PHHs support higher invasion and development rates and full LS development during long-term radical cure vaccine and drug assays. Until more rapid phenotype assessment tools are available, investigators using PHHs for LS assays will first need to screen multiple lots to find the ones most suitable for their species of interest. Fortunately, with up to 1000 aliquots of cryopreserved PHHs resulting from a production run, many thousands of individual assay units can be experimentally analyzed with the same genotypic and phenotypic background of a single suitable hepatocyte lot after identification.
Equally important to reducing the rate-limiting requirements were mitigating costs and availability of materials and automation. We estimated the cost of consumable reagents (plate, hepatocytes, medium) were less than US ~$2 per well and materials could be readily shipped to assay locations. The live portion of the assay required no robotic automation, enabling rapid implementation of the protocol at multiple laboratories including those in malaria-endemic countries. This flexibility was and will continue to be essential for developing new antimalarial PE therapies, especially against vivax malaria, since blood stages of P. vivax cannot be continuously cultured making widespread production of gametocytes for PE assays in nonendemic countries a major obstacle59. While shipment of Plasmodium spp.-infected mosquitoes from endemic countries to screening facilities is possible and was performed to generate some of these data described here, we note far greater throughput can be achieved by moving the assay itself to the endemic country to be supported by sporozoites produced from local infections. As malaria control increases worldwide, continued efforts to screen for PE therapeutics could be enabled by cryopreserved sporozoites, a concept also demonstrated in this study (Fig. 3a, Supplementary Fig. 4a, b. and Supplementary Fig. 9). Although direct comparisons were not made, our results surprisingly suggest laboratory strains of P. falciparum have reduced fitness in an in vitro LS assay.
The staining patterns with the panel of immuno-reagents used to characterize the LS morphologies in our in vitro cultures were similar to that noted in in vivo humanized mouse models, with either P. vivax or P. falciparum, confirming complete LS development in vitro31,32. In both mice and our in vitro culture, LS schizonts exhibit several large circular vacuoles of regular size, each about 1/20–1/10 the parasite total 2D area as observed under microscopy. The role and contents of these vacuoles are unknown, but high-resolution imaging revealed the membrane limiting the vacuole contained EXP2 and not UIS-4 and the internal void lacked MIF. Based on these observations, these uncharacterized vacuoles are likely a formation of the parasite membrane and not the parasitophorous vacuole membrane and would be separate from the parasite’s cytoplasm. As Plasmodium biology and morphology contains several well-characterized sequestration mechanisms (i.e., micronemes and dense granules for invasion protein machinery of sporozoites and merozoites, or the digestive vacuole for sequestration of toxic hemozoin produced during the erythrocytic stage), further characterization of the contents in these novel LS compartments could reveal interesting new drug targets such as resident solute pumps or possible toxic byproducts produced during maturation60. Morphological characterization also helps explain one of the unknowns of P. vivax lifecycle--the parasite is able to form infectious gametocytes in only days compared to over 2 weeks for P. falciparum and epidemiology studies show gametocytes are circulating within days of LS development64,65. We find a large proportion of completely mature P. vivax LS schizonts express gametocyte commitment marker Pvs16 such that all merozoites in the form are positive; while the remaining schizonts are negative for Pvs16. As commitment to gametocytogenesis has been described to begin in the asexual lifecycle producing the merozoites that will form a gamete, this stain pattern suggests whole sub-populations of P. vivax LS schizonts are producing gamete-forming merozoites instead of asexually replicating merozoites66. This mechanism, if confirmed, would help explain vivax transmission between an asymptomatic individual and the mosquito vector.
Key to the development of the next generation antimalarial toolbox, our platform is the first to perform extended ILSDA’s (days 6 or 8) in PHHs revealing not only inhibitory effects but also growth attenuation of maturing P. falciparum and P. vivax LS parasites67. Our ILSDA offers solutions to inherent issues of traditional ILSDA methods through assay standardization and high infection rates, thus greatly increasing reproducibility and sensitivity45,50,68. We show immune serum raised against SAPN-produced antibodies to FMP014/ALF (G2) and FMP014V/ALF (G6) both inhibit invasion of P. falciparum sporozoites. This finding is of high importance as FMP014V/ALF does not have PfCSP NANP repeats, indicating all inhibition comes from antibodies to the α-TSR region, thus potentially leading to longer-lived levels of protection53. Lastly, our model has the ability to screen late-stage-arresting genetically-attenuated sporozoite vaccines along with vaccine candidates targeting first generation LS merozoites entering into blood-stage.
Medium throughput small molecule screening was performed using our HCI endpoint to quantify the number and growth of LS schizonts and differentiate P. vivax schizonts from hypnozoites. Control compounds atovaquone and KDU691 behaved as expected following characterization of these compounds in vitro and in vivo42,69. We also confirmed cross-species activity of several preclinical candidate drugs to characterize the predictive value of our screen. To better understand the possible effect of host-specific metabolism, an assessment of compound efficacy in different PHH lots found no drastic PHH-specific differences for optimized compounds, including MMV390048 and atovaquone, but did find a lot-specific outcome with primaquine in relation to each lot’s CYP2D6 activity and these lots’ ability to produce the active primaquine metabolite (which cannot yet be directly quantified). In addition to differential host cell metabolism, measurement of primaquine efficacy is confounded by how quickly treated LS parasites clear from culture. Primaquine treatment in vivo has been shown to result in malformation, but not necessarily clearance, of LS parasites, while our radical cure assay was taken out to only 3 days post compound addition so as not to miss observation of schizonticidal compound activity70. To alleviate concerns of a false negative due to metabolism, dosing concentration and repetitions (maximum 10 μM administered 3 times) were optimized to provide excessive opportunity for metabolically labile compounds to act on LS parasites. Furthermore, the MMV compounds and Calibr Bioactive Library screened were all metabolism-optimized compounds, thus reducing the likelihood of a false negative due to metabolism. Despite these protocol adaptations to circumvent hepatic metabolism, we cannot rule out that our screen may miss quickly metabolized compounds. Application of our model to single point screening revealed several interesting hits, including the ionophore monensin, and suggests P. vivax schizonts and hypnozoites are sensitive to ion homeostasis. The ionophores will be best used as positive controls for radical cure assays rather than new drugs given the known problems with ionophore toxicity and poor selectivity index71. In the least, these hits demonstrate dead LS parasites can be cleared from PHH culture, and therefore drug activity can be detected, following a relatively short 3-day treatment. These ionophore hits also suggest ion homeostasis could be a viable target for anti-malarial drug discovery72.
In conclusion, for decades, preclinical malaria research on PE stages has been based on cell lines and animal models, or secondary effects from other Plasmodium lifecycle stages. We validate and promote the use of a primary hepatocyte, 384-well plate-based screening of PE therapeutic targets as an excellent resource to provide biological data and conclusions that may not be garnered from hepatoma or murine models.
Seeding 384-well plates with human hepatocytes
Individual wells of a 384-well plate (Cat No. 781091, Greiner, Monroe, NC, USA) were coated with rat tail collagen I (Cat No. 354236, Corning, New York, NY, USA) diluted to a final concentration of 5 µg collagen per cm2 in 0.02 M acetic acid, incubated at 37 °C overnight to ensure adsorption and washed thrice with 1 × PBS. Alternatively, after experimental confirmation, pre-collagen coated plates (Cat No. 781956, Greiner, Monroe, NC, USA) were used for all compound screening and a selection of ILSDA studies. For ILSDA and drug studies, cryopreserved primary human hepatocytes (Cat No. M00995-P and F00995-P, donor lots PDC, UBV, NLX) and hepatocyte culture medium (HCM) (InVitroGroTM CP Medium) were obtained from Bioreclamation IVT, Inc, (Baltimore, MD, USA). For donor screens, cryopreserved primary human hepatocytes were obtained from four companies (Cat No. M00995-P and F00995-P, donor lots E-Q, Bioreclamation IVT, Inc, Baltimore, MD, U.S.A), (Cat No. HUCSD, donor lots HUM4096A, HUM4074D, Triangle Research Labs LLC, Durham, NC, USA), (Cat No. 20-0047, donor HHF17006 lot RTA0006 and donor HHM01013 lot DFA0003, YecurisTM, Tualatin, OR, USA), (donor lot HW40, HW39, no label, Mass General Hospital, Boston, MA, USA) and maintained following manufacturer’s protocols. For HepaRG studies, NoSpin HepaRGTM, a commercially available, terminally-differentiated hepatic cell line, were seeded at 20,000 liver hepatocytes per well following the manufacturer’s instructions (Cat No. NSHPRG, Triangle Research Labs LLC, Durham, NC, USA).
All media was supplemented with a final concentration of 50 μg ml−1 penicillin-streptomycin, 100 μg ml−1 of neomycin, and 10 μg ml−1 of gentamicin. Cultures were kept on HCM (media containing serum) throughout studies as serum-containing media was found important for long-term viability. Cryopreserved PHHs were thawed following manufacturer’s protocols and viability assessed by trypan blue exclusion (typically 70–99%), resulting in recovery of 5–9 million viable cells per vial. Thawed PHHs were then diluted in HCM to a concentration of 800–900 cells per μl with 20 µl cell suspension added to individual wells. The relative number of hepatocytes seeded per well was set to achieve a confluent monolayer. At 2 days post seed each well received a complete media change (40–50 µl), then media was changed per the experimental protocol (Fig. 1b).
Hepatocyte functional assays
Albumin and Factor IX production were measured by collecting media from hepatocytes (PDC) seeded wells at set time points and then storing samples at −80 °C until collection was completed. For albumin measurements, 12 wells (at 50 μl volume) were collected every 2 days for 30 days with media addition after time point removal. Albumin measurements (ng m−1) were collected using the Albumin (human) AlphaLISA Detection kit specific for the EnSpire Alpha screen (Cat No. AL294C, Perkin Elmer, Waltham, MA, USA) and the mean with s.d. (n = 6) were reported. Samples (n = 3) were quantified for Factor IX ELISA per manufacturer’s protocols (Cat No. EF1009-1, AssayPro, St. Charles, MO, USA). Cyotchrome P450 3a4 induction was measured using CYP3A4 P450 Glo™ luciferin-IPA kit (Cat No. V9002, Promega, Madison, WI, USA). Hepatocytes were induced for 72 h with 25 μM Rifampicin (Cat No. BP26795, Fisher, Hampton, NH, USA) in plate media, or an equivalent volume of DMSO in uninduced controls, and luciferin signal measured by a luminance plate reader following the lytic version of the manufacturer’s protocol. Basal enzymatic characterization was performed for all 14 BIVT donor lots and provided by Bioreclamation IVT, Inc (Baltimore, MD, USA). Metabolic assays were run in triplicate and results represent the average of the 3 samples (Supplementary Table 2 and Supplementary Fig. 5). Activity results were analyzed by HPLC-UV or LC/MS/MS validated procedures. Metabolite formation for all enzymes was measured after a 60 min. Cell incubation at 37 °C, 5% CO2 resulting in a final concentration of 1 million cells per ml. The standard 60 min incubation was used for this assay.
Live imaging and analysis of hepatobiliary formation
A total of 6 time points (day 2, 4, 8, 14, 21, 30) with experimental replicate wells (n = 3, n′ = 3) were selected to phenotypically assess the PHHs (donor lot PDC) seeded in the commercial 384-well plate (Fig. 2a). For the Bioreclamation IVT PHH donor screen, a total of 4 time points (day 2, 4, 8, 14) with experimental replicate wells (n = 1, n′ = 3) were selected to phenotypically assess the PHHs seeded in the commercial 384-well plate (Supplementary Table 3). Wells were stained for 45 min at 37 °C and 5% CO2 with staining solution diluted in phenol-free, serum-free RPMI containing 10 μM Hoechst 33342 (Cat No. H3570, Life Technologies, Carlsbad, CA, USA), 750 nM Tetramethylrhodamine (TMRM) (Cat No. T668, Life Technologies, Carlsbad, CA, U.S.A.) and 4 μM CellTrackerTM Green CMFDA dye (Cat No. C7025, Life Technologies, Carlsbad, CA, USA). An Operetta high-content imaging machine (Perkin Elmer, Waltham, MA, USA) was used in wide field mode (×20 objective, 0.4 NA) to capture 35 tiles within each 384-well while simultaneously acquiring 4 channels (Transmitted, TRITC, FITC, DAPI) representing brightfield, respiration, transport, and viability. A z-plane stack of −2 to 10 μm with a 2 μm plane distance was acquired for each well. Using the Harmony software (version 4.1), a maximum image projection merging all z-planes was formatted for each well per time point. First, total hepatocytes per well were calculated by using Hoechst staining of hepatocyte nuclei where populations termed “healthy” and “unhealthy” were determined by area (µm2) and MFI ≥ 3000. Next, the area and fluorescent intensity of TMRM was calculated using the emitted fluorescence (TRITC channel) where the MFI of entire well was used to compare mitochondrial activity between the time points.
To accurately find and classify the bile canaliculi as active or inactive transport, a combination of several building blocks and image filter sets were required using Harmony software (4.1) (Supplementary Fig. 2). Post compilation of the z-stack, a Gaussian image filter was applied to enrich contrast of active bile canaliculi and normalize background intensity. Simultaneously, the image was filtered selecting for intensity of the FITC channel allowing for identification of hepatocyte cells incapable of transporting dye. An image calculation was applied (Gaussian filtered image plus filtered FITC channel) and the following criteria were obtained for all classified bile canaliculi at all time points; morphology (length, width, area, roundness), and intensity (sum, mean, maximum, minimum). Thresholds to distinguish between the populations were set based on MFI ( ≥ 3000), area (active ≥ 10 µm2, inactive ≥ 5 µm2), and roundness (active ≤ 0.83, inactive ≥ 0.83) to classify all bile canaliculi as either inactive or active transport.
Lastly, composite images of mitochondrial activity and bile canaliculi were created in the open access image analysis platform, FIJI, using a macro to assign color to TMRM intensity ranges with maximum projections of MFI bile canaliculi images superimposed in 8-bit gray scale73. The FIJI plugin, Coloc2, was used to generate Mander’s correlations for above zero intensity of channel (M1, M2) and above auto threshold of channel (tM1, tM2) for whole images (×20, 0.4 NA) and Pearson’s correlation, r, for selected regions of interest (ROI) for days 2–30. Run parameters were set with a point spread function (PSF) at 3 and Costes randomizations at 100, allowing for minimal influence of noise and independent of image brightness36,37.
P. falciparum mosquito infections from in vitro culture
P. falciparum (strain NF54) was maintained according to standard methods at 37 °C (5% O2 and 5% CO2, nitrogen balanced) in 5% hematocrit (O + blood), 10% AB human serum (The Interstate Blood Bank INC, Memphis, TN, USA), RPMI 1640 medium (Cat No. CUS-0645, KD medical, Columbia, MD, USA), and 2.5% sodium bicarbonate74. Two gametocyte cultures were started three days apart using standard methods and an aliquot of each was mixed together when stage V gametocytes were prevalent (day 14–17 of gametocyte cultures) and used to infect day 4–6 old mosquitoes. Infections of laboratory-reared Anopheles (An.) stephensi (Nijmegen strain) were accomplished using a temperature-controlled Hemotek membrane-feeding device (Discovery Workshops, Accrington, UK) and kept at 80% humidity in 26 °C environmental chambers with 10% sucrose supplemented water75. Additionally, P. falciparum (strains NF54-WT and NF54-GFP) infected An. stephensi mosquitoes were shipped live from John Hopkins University Malaria Research Institute (JHUMRI) insectary and parasitology core (Baltimore, MD, USA) on day 10 post-infection and maintained at 80% humidity in 26 °C environmental chambers with 10% sucrose supplemented water. Salivary glands of mosquitoes 14–16 days after infection were aseptically dissected and collected into Schneider’s media (Cat No. S9895, Sigma-Aldrich, St. Louis, MO, USA)76.
The Human subjects protocols for this study was approved by the Institutional Ethics Committee of the Thai Ministry of Public Health, the Human Subjects Research Review Board of the U.S. Army (WRAIR#1949), Ethical Review Committee of Faculty of Tropical Medicine, Mahidol University (TMEC 11-008 and 14–016), the Oxford Tropical Medicine Ethical Committee, Oxford University, England (OxTREC 17-11 and 40–14), and the Cambodian National Ethics Committee for Health Research (101NECHR). The protocols conformed to the Helsinki Declaration on ethical principles for medical research involving human subjects (version 2002) and informed written consent was obtained for all volunteers.
P. vivax mosquito infections from infected patients
Isolates of P. vivax were collected from symptomatic patients enrolled in the study after giving written informed consent at the Thai malaria clinic (SMRU) in Tak province, Mae Sod Malaria Clinic (Thailand Ministry of Public Health) in Tak province, and through recruitment via the village malaria workers network and the local health centers in the Mundolkiri Province in Cambodia. A sample of P. vivax-infected blood was drawn by venipuncture into heparin tubes. Thick and thin Giemsa-stained smears were prepared after removal of white blood cells (WBCs). A diagnostic PCR was used to confirm microscopic identification that P. vivax was the only Plasmodium species present in the samples used for the study77.
The mosquito infections for P. vivax were performed using a colony of An. dirus (Bangkok strain), An. cracens78 or An. dirus B in Cambodia. Briefly, 150 μL of RBC pellet from infected patient blood samples was suspended in pooled normal AB human serum to 50% hematocrit. Next, 300 μL of the suspension was fed for 30 min to 5–7 days old female mosquitoes via an artificial membrane attached to a water-jacketed glass feeder maintained at 37 °C. Engorged mosquitoes were kept on 10% sucrose solution and maintained at 26 °C and 80% humidity until dissected. Salivary glands of mosquitoes 14–16 days after infection were dissected and collected as described above. Studies including freshly dissected P. vivax sporozoites were performed at Armed Forces Research Institute of Medical Sciences, Bangkok, Thailand, Shoklo Malaria Research Unit, Mae Sot, Thailand, and Institut Pasteur du Cambodge, Phnom Penh, Cambodia. For some LS studies, mosquitoes carrying P. vivax oocysts were shipped, still pre-infectious, from AFRIMS to the University of South Florida following permit approval by the Thai Ministry of Health, US Center for Disease Control, US Department of Agriculture, and Florida Department of Agriculture.
Infection with cryopreserved Plasmodium sporozoites
Previously cryopreserved lots of P. vivax and P. falciparum sporozoites were used to assess PHH invasion and development. Cryopreservation of sporozoites were performed following previously published protocols and thawed at room temperature with dilution in HCM51,52. A lot of cryopreserved P. vivax sporozoites refers to a single patient derived case while a lot of cryopreserved P. falciparum sporozoites refers to lab-adapted strain NF54. A cryopreserved P. vivax sporozoite lot was used and infected at 2.0 × 104 sporozoites per well (Supplementary Fig. 4a, b, Supplementary Fig. 9, and Supplementary Table 1) or at 1.0 × 104 sporozoites per well (Fig. 3a and Supplementary Table 3). A cryopreserved P. falciparum sporozoite lot was used and infected at 2.5 × 104 sporozoites per well (Fig. 3a and Supplementary Table 3).
Inhibition of Liver Stage Development Assays (ILSDAs)
After salivary gland dissections at WRAIR, SMRU, IPC, or USF, sporozoites were counted using a hemocytometer and diluted accordingly in HCM. For antibody and serum exposure, sporozoites were incubated with test serum samples in a serially diluted manner (1:2, 1:4, 1:8, 1:16, 1:32, 1:64, 1:128, 1:256 in HCM) or with monoclonal antibodies (80, 40, 20, 10, 5, 2.5, 1.25, 0.25 µg ml−1 in HCM) (P. falciparum) and 250, 25, 2.5, 0.25 µg ml−1 (P. vivax) for 20 min at room temperature or overnight at 37 °C, 5% CO2. For experimental control, sporozoites were exposed to pre-bleed mouse sera as well as in absence of an exposure (HCM only) then held at room temperature for 20 min or overnight at 37 °C, 5% CO2. After incubation, 1.0 × 104 or 1.8 × 104 sporozoites from each condition were added to wells in duplicates or triplicates, spun down at 200 × g for 5 min, and allowed to invade for 24 h at 37 °C before washing with HCM. Media was changed every 2 days using HCM supplemented with antimicrobial mix until fixation 6 days post initiation.
P. vivax and P. falciparum antimalarial drug studies
As stated previously, salivary glands were disrupted and sporozoites were counted on a hemocytometer, diluted in HCM, and 0.5 × 104 added per well prior to centrifugation at 200 × g for 5 min. Drug regimen was defined by treatment mode, prophylactic or radical cure, with addition of drug on assigned days and HCM supplemented with antimicrobials replenished daily. Compounds were then dissolved in 100% DSMO to stock concentrations of 10 mM and then dispensed and serially diluted in absorption resistant 384-well master plates (Axygen, Tewksbury, MA, USA) using a multichannel pipette. Plated compounds were stored at −80 °C before and after shipment to an endemic laboratory (SMRU in Thailand and IPC in Cambodia) on dry ice. Plated compounds were thawed at room temperature, spun down at 200 × g for 5 min and stored covered with foil tape in an ambient desiccation chamber between daily transfers. Transfer of compounds from the master plate to the 384-well assay microplate was performed using a sterilized, custom made, manual pin tool (VP Scientific, San Diego, CA, USA) engineered to dispense 40 nL of liquid per pin into 40 μL HCM volume in the well to achieve a 1000-fold dilution. Before and after compound transfer the pin tool was cleaned by two wash cycles (dip and blot) in each of 50% DMSO in water, then 70% EtOH in water, then VP clean solution, then water, and finally 100% MeOH, per manufacturer’s protocols. Initially, compounds were tested in independent experiments using an 8-point concentration format with 3-fold dilutions (final concentrations of 10 µM to 5 nM). For Single Point assays, compounds were tested and the most potent 24 hits were selected for confirmation and EC50 determination in the same 8-point concentration format described above. For each assay plate, both a positive (KDU691) and negative (0.1% DMSO) control were added and a minimum of 8 wells per plate were analyzed. Based on controls, a Z′ factor was calculated for each plate and positive value were considered acceptable for data analysis79.
Automated image acquisition and data analysis
At 5−8 days post infection, wells were fixed with 4% paraformaldehyde (PFA) for 10 min at room temperature and washed twice with 1×PBS. For P. falciparum experiments, wells were incubated in blocking buffer (0.03% TritonX-100, 1% (w/v) BSA in 1 × PBS) with mouse anti-GADPH (3.2 µg ml−1, 1:50,000 dilution) overnight at 4 °C. For P. vivax experiments, wells were incubated in blocking buffer with polyclonal rabbit or mouse recombinant anti-UIS4 mAB (1 µg ml−1, 1:5000 or 1:25,000-fold dilution) overnight at 4 °C. After, the wells were washed thrice with 1× PBS and incubated for 1 h at room temperature with either goat anti-rabbit or goat anti-mouse Alexa Fluor® 488 conjugate (2 µg ml−1, 1:1000-fold dilution; Cat No. A11001, Molecular Probes, ThermoFisher, Waltham, MA, USA) secondary antibody and Hoechst (10 µg ml−1, 1:1000-fold dilution) then washed thrice, and filled with 1× PBS for imaging and storage.
Imaging and data analysis of the ILSDAs and drug plates were completed using the Operetta Imaging System and Harmony software 4.1 (Perkin Elmer, Waltham, MA, USA) or ImageXpress and MetaXpress software (Molecular Devices, Sunnyvale, CA, USA). Images were acquired using FITC, DAPI, and brightfield channels at ×20 magnification meaning each well of a 384-well plate is 35 fields of view, tiled together. After image acquisition, hepatocyte nuclei were counted with the DAPI channel and objects greater than 30 μm2 were defined by the software. Parasites were counted with the FITC channel and were identified by area, mean intensity, maximum intensity and cell roundness. To improve the accuracy of the software identifying the parasites, parasites were separated into 2 populations: small and large forms with the large forms divided into 5 subpopulations. The parameters and thresholds used to count the parasites are summarized in Table 1. After the parasites were counted, the five subpopulations of large forms were added together for P. vivax and the small and large forms were added for P. falciparum. Drug EC50 curves and % inhibition were generated using total population counts and parasite size where controls were calculated as the average of replicates (when performed) using the Levenberg-Marquardt algorithm, using KDU691 as the normalization control, as defined in CDD Vault (Burlingame, CA, USA). Similarly, IC50 curves and % inhibition of ILSDAs was performed using dose-response modeling in Prism (Graphpad, La Jolla, CA, USA) where data were normalized to the negative control (infected well, ICtrl) described by the equation below:
where X is the measured inhibition by the antibody or immune sera and ICtrl is calculated using the average of 12 experimental replicates in the same 384-well plate.
High-resolution imaging and blood breakthrough assays
Briefly, the same immunofluorescence assay (IFA) protocol was followed above with the following fold dilutions of monoclonal antibodies obtained from The European Malaria Reagent Repository: mouse anti-GAPDH (Cat No. 7.2) at 1:50,000, mouse anti-EXP1and EXP2 (Cat No. 5.1 and 7.7) at 1:1000, mouse anti-GLURP (clones 22G6, 8B12, 2C7) at 1:200, anti-MSP1 (Cat No. 12.10) at 1:200, and anti-MSP2 (Cat No. 12.3) at 1:20039,40,41. The following antibodies were used; polyclonal rabbit anti-UIS-4 at 1:5000, recombinant mouse UIS-4 at 1:25,000, polyclonal rabbit anti-MIF 1:1000, and monoclonal mouse ACP at 1:1000 and were obtained from Center for Infectious Disease Reasearch, WA, USA31. The anti-UIS4 recombinant monoclonal antibody used in this study was derived from a hybridoma expressing anti-UIS4 monoclonal antibody developed by methods previously described31,80. We produced recombinant mouse anti-Pvs16 then conjugated to Alexafluor® 647 and used experimental dilutions at 1:50 (Cat No. A20186, Molecular Probes, ThermoFisher, Waltham, MA, USA). We also produced a mouse anti-HSP70 hybridoma supernatant (clone 4C9) and used at 1:100. After primary staining, the wells were washed thrice with 1× PBS and incubated for 1 h at room temperature with either goat anti-rabbit Alexa Fluor® 488 conjugate, goat anti-mouse Alexa Fluor® 488 conjugate, goat anti-rabbit Alexa Fluor® 568, or goat anti-mouse Alexa Fluor® 568 conjugate (2 µg ml−1, 1:1000-fold dilution; Cat No. A11001, A11034, A11004, A11011, Molecular Probes, ThermoFisher, Waltham, MA, USA) secondary antibody and Hoechst (10 µg ml−1, 1:1000-fold dilution) then washed thrice, and filled with 1× PBS for imaging and storage. High-resolution, z-stacked images of P. vivax and P. falciparum LS parasites were captured with a ×100 oil objective, 1.4 NA on a DeltaVision Core system (GE Healthcare Life Sciences, Piscataway Township, NJ, USA). Images were deconvoluted using the softWoRx® image analysis package (GE Healthcare Life Sciences, Piscataway Township, NJ, USA) and z-stacks with added scale bars were processed in FIJI73. Images captured with secondary antibody Alexa Fluor® 568 were re-colored to magenta using FIJI in order to meet publication image standards.
Plasmodium blood breakthrough studies were performed using either fresh reticulocytes prepared from Duffy antigen positive buffy packs (P. vivax) or fresh O+ whole blood (The Interstate Blood Bank INC, Memphis, TN, USA). O+ blood (25 ml) was centrifuged at 2000 RCF for 5 min to remove buffy coat and RBCs were washed thrice with incomplete (no serum or sodium bicarbonate) RPMI 1640 medium (Cat No. CUS-0645, KD medical, Columbia, MD, USA). Similarly, buffy pack blood (60–70 ml) was washed with McCoy’s 5A incomplete medium (Cat No. M9309, Sigma-Aldrich, St. Louis, MO, USA), filtered on a NEO1 Leukocyte Reduction filter (Cat No. BPF4, Haemonetics, Braintree, MA, USA) then subjected to a CD71+ immuno-magnetic purification following manufacturer’s specifications (Miltenyi Biotech, Bergisch Gladbach, Germany). CD71+ selected cells were washed in McCoy’s 5A incomplete medium and New Methylene Blue thin blood smears were performed to check for purity, yielding normally >95%. Reticulocytes and RBCs were kept for up to 7 days at 4 °C at 50% haematocrit in incomplete medium before overlay on mature LS cultures; days 9–12 for P. vivax and days 6–8 for P. falciparum. Prior to addition to LS cultures, reticulocytes or RBCs were pelleted and resuspended in serum containing media then cultures were co-incubated overnight at 37 °C, 5% CO2 after pipette disruption. Smears were collected daily and fixed with methanol or Giemsa stained.
All graph bars are represented by means with standard deviation (s.d.). Significance of mean was assessed by one-way ANOVA with Dunnett’s multiple comparisons (Fig. 2, Fig. 6e, Supplementary Figure 4a, b), one-way ANOVA (nonparametric) followed by Dunn’s multiple comparison (Supplementary Figure 4c, d), two-way ANOVA with Dunnett’s multiple comparisons (Fig. 3a, b, Supplementary Figure 4), two-way ANOVA with Tukey’s multiple comparisons (Fig. 6b) When standard deviation is reported, n represents biological replicates where n′ represents experimental replicates per biological replicate.
The data that support the findings of this study are available from the corresponding author upon request.
Material has been reviewed by the Walter Reed Army Institute of Research. There is no objection to its presentation and/or publication. The opinions or assertions contained herein are the private views of the authors, and are not to be construed as official, or as reflecting true views of the Department of the Army or the Department of Defense. The investigators have adhered to the policies for protection of human subjects, as prescribed in AR 70–25.
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We thank the P. vivax patients and residents of Tak Province, Thailand and Mondulkiri Province, Cambodia for their generosity for participation in the study. We thank AFRIMS, SMRU, and IPC insectary department and staff for An. dirus mosquito breeding, feeding of P. vivax infected blood, and maintenance. Shoklo Malaria Research Unit is part of the Mahidol Oxford University Research Unit, supported by the Wellcome Trust of Great Britain (F.N.). We acknowledge John Hopkins University Malaria Research Institute (JHUMRI) insectary and parasitology core, with special thanks to A. Tripathi and P. Sinnis for facilitating shipments of P. falciparum-infected mosquitoes (J.H.A.). The following reagent obtained through BEI Resources, NIAID, NIH: Monoclonal Antibody 2A10 Anti-P. falciparum Circumsporozoite Protein (CSP), MRA-183A, Hybridoma 2F2 Anti-P. vivax CSP, MRA-184, and Hybridoma 2E10.E9 Anti-P. vivax CSP, MRA-185, contributed by E. Nardin. Monoclonal antibodies 12.10 (anti-MSP1), 5.1 (anti-EXP1), 7.7 (anti-EXP2), clones 22G6, 8B12, 2C7 (anti-GLURP), and 7.2 (anti-GAPDH) were obtained from The European Malaria Reagent Repository (http://www.malariaresearch.eu). HCI data from drug studies was produced in collaboration with the Biomedical Microscopy Core at the University of Georgia (D.E.K.). Funding support was provided by Bill and Melinda Gates Foundation (OPP1023643 to J.H.A., OPP1023601 to D.E.K), Medicines for Malaria Venture (RD/16/1082 and RD/15/022 to D.E.K., RD/2017/0042 to B.W. and A.V.), the Georgia Research Alliance (D.E.K.), and National Institutes of Health (R01AI064478, BAA-NIAID-DAIT-NIHAI2013164 to J.H.A.).
The authors declare no competing interests.
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Roth, A., Maher, S.P., Conway, A.J. et al. A comprehensive model for assessment of liver stage therapies targeting Plasmodium vivax and Plasmodium falciparum. Nat Commun 9, 1837 (2018). https://doi.org/10.1038/s41467-018-04221-9
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