Rodent malaria

Malaria parasites that infect rodents (mice and rats) have been extensively used to study and model human disease in vivo. Four species of rodent malaria parasites (RMPs i.e. P. berghei, P. yoelii, P. chabaudi, P. vinckei) that were originally isolated on various occasions in Central African thicket rats have been at the centre of these studies. These parasite species share a highly conserved chromosomal gene synteny with the human infecting P. falciparum (Carlton et al., Reference Carlton, Vinkenoog, Waters and Walliker1998b) with, however, subtle differences in stage-specific morphologies, duration of life cycle and host cell preferences (Table 1). P. chabaudi and P. vinckei have the ability to invade mature red blood cells and achieve high parasitaemia just like human P. falciparum and P. malariae, whilst P. berghei and P. yoelii are generally restricted to reticulocyte invasion which is similar to human infecting P. vivax and P. ovale (Table 1). Nevertheless, the basic biology of rodent- and human-infectious Plasmodium is fundamentally conserved. This has allowed for their use in studying several aspects of malaria parasite development, host–pathogen interactions, drug efficacy evaluations and vaccine studies which would otherwise be inaccessible with P. falciparum in vitro. Furthermore, RMPs offer a plethora of advantages among which include their ease of handling in rodents, experimental tractability of all life cycle stages under lab conditions as well as the availability of a wide array of genetic manipulation systems. Still, RMPs and their hosts are both divergent from their human equivalents (P. falciparum and humans) (Fig. 2). Even though they can provide crucial insights into the conserved elements of parasite biology, the finer molecular details might be different from their human counterparts due to the unique aspects of their hosts. The use of these models should therefore be pertinently tailored to the biological question under study through direct comparison to human parasites (Craig et al., Reference Craig, Grau, Janse, Kazura, Milner, Barnwell, Turner and Langhorne2012; De Niz and Heussler, Reference De Niz and Heussler2018).

Fig. 2.

Phylogenetic relatedness of Plasmodium's spp. The tree is based on recent published genomes of the indicated Plasmodium spp. and was adapted with minor modifications from Rutledge et al. (Reference Rutledge, Böhme, Sanders, Reid, Cotton, Maiga-Ascofare, Djimdé, Apinjoh, Amenga-Etego, Manske, Barnwell, Renaud, Ollomo, Prugnolle, Anstey, Auburn, Price, McCarthy, Kwiatkowski, Newbold, Berriman and Otto2017), Böhme et al. (Reference Böhme, Otto, Cotton, Steinbiss, Sanders, Oyola, Nicot, Gandon, Patra, Herd, Bushell, Modrzynska, Billker, Vinetz, Rivero, Newbold and Berriman2018).

Table 1.

Comparison of human, rodent and primate Plasmodium's in relation to key life cycle features, host tropisms and disease pathogenesis

NHPs malaria

For decades, NHPs have also proved invaluable to studying malaria disease pathogenesis as well as fundamental aspects of parasite biology, reviewed by Galinski and Barnwell (Reference Galinski, Barnwell, Abee, Mansfield, Tardif and Morris2012). Crucially, P. cynomolgi and P. vivax hypnozoites (dormant liver stages) were first discovered in NHPs, specifically in rhesus macaques for the former (Krotoski et al., Reference Krotoski, Garnham, Bray, Krotoski, Killick-Kendrick, Draper, Targett and Guy1982b) and in Chimpanzees for the latter (Krotoski et al., Reference Krotoski, Collins, Bray, Garnham, Cogswell, Gwadz, Killick-Kendrick, Wolf, Sinden, Koontz and Stanfill1982a). Due to a reticulocyte invasion dependency (Gruszczyk et al., Reference Gruszczyk, Kanjee, Chan, Menant, Malleret, Lim, Schmidt, Mok, Lin, Pearson, Rangel, Smith, Call, Weekes, Griffin, Murphy, Abraham, Sriprawat, Menezes, Ferreira, Russell, Renia, Duraisingh and Tham2018; Malleret et al., Reference Malleret, El Sahili, Tay, Carissimo, Ong, Novera, Lin, Suwanarusk, Kosaisavee, Chu, Sinha, Howland, Fan, Gruszczyk, Tham, Colin, Maurer-Stroh, Snounou, Ng, Chan, Chacko, Lescar, Chandramohanadas, Nosten, Russell and Rénia2021) (Table 1), P. vivax lacks a robust in vitro culture system unlike P. falciparum. NHPs have thus been instrumental for understanding the biology of this parasite. Over 40 P. vivax strains that are able to infect NHPs, specifically New World monkeys of the Aotus and Saimiri species have been archived by the CDC (Galinski and Barnwell, Reference Galinski, Barnwell, Abee, Mansfield, Tardif and Morris2012). By infecting splenectomized NHPs (to minimize splenic clearance of infected red blood cells) through mosquito bites or intravenous injection of purified sporozoites, chronic relapsing P. vivax malaria can be reproduced in these models (Joyner et al., Reference Joyner, Barnwell and Galinski2015). However, due to difficulties in isolating enough sporozoites from P. vivax, a closely related sister species, P. cynomolgi (Fig. 2) is often used as a model for P. vivax in NHPs as this parasite can be used to generate millions of sporozoites within a short period of time (Rosenberg and Rungsiwongse, Reference Rosenberg and Rungsiwongse1991; Joyner et al., Reference Joyner, Barnwell and Galinski2015). P. cynomolgi and P. vivax share a highly conserved genome organization (GC content ~41%, equal number of positionally conserved centromeres etc) (Tachibana et al., Reference Tachibana, Sullivan, Kawai, Nakamura, Kim, Goto, Arisue, Palacpac, Honma, Yagi, Tougan, Katakai, Kaneko, Mita, Kita, Yasutomi, Sutton, Shakhbatyan, Horii, Yasunaga, Barnwell, Escalante, Carlton and Tanabe2012) as well as similar features of disease pathology such as the formation of hypnozoites. Unlike P. vivax which is mostly restricted to New World monkeys, P. cynomolgi strains that infect larger Old World monkeys (macaques) have been successfully adapted providing, in the absence of long-term in vitro culture, the only means to generate sufficient amounts of parasite material for downstream analyses (Joyner et al., Reference Joyner, Barnwell and Galinski2015). Moreover, P. cynomolgi is easily amenable to genetic manipulation systems allowing for interrogation of gene function systems which have largely been inaccessible in P. vivax (Voorberg-van der Wel et al., Reference Voorberg-van der Wel, Zeeman, van Amsterdam, van den Berg, Klooster, Iwanaga, Janse, van Gemert, Sauerwein, Beenhakker, Koopman, Thomas and Kocken2013; Joyner et al., Reference Joyner, Barnwell and Galinski2015). P. cynomolgi remains the main model of understanding P. vivax biology among which include evaluating the efficacy of antimalarial drugs with potential activity in difficult to eliminate hypnozoite stages, reviewed by Zeeman and Kocken (Reference Zeeman and Kocken2017).

Other NHP infecting malaria parasites include P. coatneyi and P. knowlesi. P. coatneyi was first isolated in the early 1960s from a forest mosquito Anopheles hackeri in Malaysia (Eyles et al., Reference Eyles, Fong, Warren, Guinn, Sandosham and Wharton1962). Only one isolate of P. coatneyi (the Hackeri strain) has been characterized and preserved by the CDC ever since (Galinski and Barnwell, Reference Galinski, Barnwell, Abee, Mansfield, Tardif and Morris2012). In macaques, P. coatneyi infection is highly similar to P. falciparum, sharing almost the same aspects of parasite morphology and disease pathogenesis. Late stages of P. coatneyi (trophozoites and schizonts) are known to sequester in tissues and organs just like human P. falciparum. P. coatneyi infected red blood cells also exhibit rosetting characteristics as is commonly seen in P. falciparum (Udomsangpetch et al., Reference Udomsangpetch, Brown, Smith and Webster1991). Crucially, most features of severe malaria pathogenesis; high parasitaemia, anaemia, parasite tissue sequestration, coma and cerebral malaria are all known to occur in P. coatneyi infected NHPs. This has made this species of Plasmodium a suitable model for a comparative analysis of human malaria disease pathogenesis despite a lack of close intrinsic genetic similarity (Mitsui et al., Reference Mitsui, Arisue, Sakihama, Inagaki, Horii, Hasegawa, Tanabe and Hashimoto2010) (Fig. 2). A zoonotic Plasmodium, P. knowlesi is another NHP infecting malaria parasite which was first isolated in the 1930s (H, Nuri, Hackeri strains) in macaques (Galinski and Barnwell, Reference Galinski, Barnwell, Abee, Mansfield, Tardif and Morris2012). P. knowlesi is the only NHP malaria parasite with a relatively short life cycle (24 h) that often results in a rapid increase in parasitaemia and death of the host in the absence of treatment. Even though this parasite can infect humans, in what has been some of the best-described cases of zoonotic malaria (Singh and Daneshvar, Reference Singh and Daneshvar2013), differences in the duration of life cycle and disease presentation has restricted the utility of P. knowlesi as a model of P. falciparum. Nevertheless, P. knowlesi infections in macaques have been used to study host immunity to malaria, merozoite invasion biology as well as antigenic variation mechanisms (Galinski and Barnwell, Reference Galinski, Barnwell, Abee, Mansfield, Tardif and Morris2012; Singh and Daneshvar, Reference Singh and Daneshvar2013). In fact, the first merozoite invasion receptor ligands on the surface of host red blood cells, Duffy group antigens, were identified using this species of Plasmodium (Miller et al., Reference Miller, Mason, Dvorak, McGinniss and Rothman1975).

Other Plasmodium spp. in animals

Before the discovery of RMPs (P. berghei in 1949), avian malaria parasites were the experimental spp. of choice for studying malaria parasite biology as they were discovered at almost the same time as P. falciparum (Huff and Bloom, Reference Huff and Bloom1935; Raffaele and World Health, Reference Raffaele1965; Pigeault et al., Reference Pigeault, Vézilier, Cornet, Zélé, Nicot, Perret, Gandon and Rivero2015b). Avian malaria parasites comprise of an unknown number of species (>55) belonging to two genera, Plasmodium and Haemoproteus (Atkinson et al., Reference Atkinson, Dusek, Woods and Iko2000; Valkiūnas and Iezhova, Reference Valkiūnas and Iezhova2018). Meanwhile, avian malaria is mostly caused by P. relictum (subgenera Haemamoeba) which is endemic to all parts of the world except Antarctica (Bensch et al., Reference Bensch, Hellgren and Pérez-Tris2009). Other causative agents include P. gallinaceum and P. lophurae which occur at less frequency and can be a significant problem in poultry industries (Coggeshall, Reference Coggeshall1938; Springer, Reference Springer1991). Despite conserved life cycle features with other Plasmodium, avian malaria parasites have a slightly different life cycle. They display a low host specificity across bird species as well as a marked variation in developmental patterns in various hosts (Bensch et al., Reference Bensch, Hellgren and Pérez-Tris2009; Hellgren et al., Reference Hellgren, Atkinson, Bensch, Albayrak, Dimitrov, Ewen, Kim, Lima, Martin, Palinauskas, Ricklefs, Sehgal, Valkiūnas, Tsuda and Marzal2015). Avian malaria parasites also appear to produce dormant parasite forms both in the liver and ABS cycles as opposed to other Plasmodium such as P. vivax which produce the same only during the liver stage (Cosgrove, Reference Cosgrove2005). Moreover, avian red blood cells are nucleated. This provides steady access to nutrients and metabolite transport mechanisms (through the host) which would obviously contribute to divergent evolutionary trajectories of these parasites as compared to their mammalian counterparts (Böhme et al., Reference Böhme, Otto, Cotton, Steinbiss, Sanders, Oyola, Nicot, Gandon, Patra, Herd, Bushell, Modrzynska, Billker, Vinetz, Rivero, Newbold and Berriman2018). Broadly, avian malaria is usually sublethal (in endemic areas) while in some cases it can lead to severe disease especially in cases of accidental introduction in non-endemic areas (Atkinson et al., Reference Atkinson, Dusek, Woods and Iko2000). After the discovery of RMPs, experimental malaria almost, entirely, switched to rodents (Rivero and Gandon, Reference Rivero and Gandon2018). However, in recent years, avian malaria parasites have re-emerged as appropriate models to studying malaria parasite ecology and evolution mostly due to their rich genetic and phenotypic diversities (Pigeault et al., Reference Pigeault, Nicot, Gandon and Rivero2015a, Reference Pigeault, Vézilier, Cornet, Zélé, Nicot, Perret, Gandon and Rivero2015b; Rivero and Gandon, Reference Rivero and Gandon2018). Complete genomes for P. relictum and P. gallinaceum have now been published (Böhme et al., Reference Böhme, Otto, Cotton, Steinbiss, Sanders, Oyola, Nicot, Gandon, Patra, Herd, Bushell, Modrzynska, Billker, Vinetz, Rivero, Newbold and Berriman2018). Avian malaria parasites have also played some vital historical role not just in understanding parasite ecology and evolution but also technology development. In fact, the first genetic transformation of a malaria parasite was achieved in P. gallinaceum (Goonewardene et al., Reference Goonewardene, Daily, Kaslow, Sullivan, Duffy, Carter, Mendis and Wirth1993).

Pathogenesis of severe malaria

In humans, malaria disease spectrum varies significantly between children and adults. These differences can range from no symptoms at all in asymptomatic individuals, mild disease in some and in a few cases (<2%) severe and lethal forms of the disease. Severe malaria is often characterized by a multi-organ system involvement presenting as anaemia, metabolic acidosis or cerebral malaria (CM) (Miller et al., Reference Miller, Baruch, Marsh and Doumbo2002). CM remains the leading cause of malaria-related deaths in children under the age of five in SSA (Ghazanfari et al., Reference Ghazanfari, Mueller and Heath2018). Irrespective of successful antimalarial treatment, >15% mortality rates occur in CM patients (Newton and Krishna, Reference Newton and Krishna1998). In areas of low malaria transmission like SEA, CM does not just occur in children as the disease is also common in adults (Ghazanfari et al., Reference Ghazanfari, Mueller and Heath2018). Despite intensive research efforts, the pathogenesis of CM remains poorly understood. Studies using post-mortem samples have, however, pointed to tissue and organ sequestration of parasite-infected red blood cells as a pathological hallmark of all human CM cases (Berendt et al., Reference Berendt, Tumer and Newbold1994; Taylor et al., Reference Taylor, Fu, Carr, Whitten, Mueller, Fosiko, Lewallen, Liomba and Molyneux2004). Sequestration of infected red blood cells to the vascular endothelium of tissues is mediated by a parasite ligand expressed on the surface of red blood cells, the polymorphic P. falciparum erythrocyte membrane protein-1 (PfEMP-1) that undergoes antigenic variation (Jensen et al., Reference Jensen, Adams and Hviid2020). Several host endothelial receptors bound by different forms of PfEMP-1 have been identified among which include CD36, the intercellular adhesion molecule 1 (ICAM-1) and the endothelial protein C receptor (EPCR) (Berendt et al., Reference Berendt, Simmons, Tansey, Newbold and Marsh1989; Gamain et al., Reference Gamain, Gratepanche, Miller and Baruch2002; Brown et al., Reference Brown, Turner, Christoffersen, Andrews, Szestak, Zhao, Larsen, Craig and Higgins2013; Avril et al., Reference Avril, Bernabeu, Benjamin, Brazier and Smith2016). It has been proposed that parasite sequestration through PfEMP-1 engagement of host receptors causes a mechanical occlusion of blood vessels which reduces blood flow and delivery of oxygen and nutrients into various tissues and organs. In CM, this has been associated with hypoxia, coma and death, the classical clinical features of the disease (Taylor et al., Reference Taylor, Fu, Carr, Whitten, Mueller, Fosiko, Lewallen, Liomba and Molyneux2004). However, besides parasite sequestration, immune effector cells and platelet accumulation also appear to be important drivers of CM pathogenesis (Grau et al., Reference Grau, Mackenzie, Carr, Redard, Pizzolato, Allasia, Cataldo, Taylor and Molyneux2003; Hochman et al., Reference Hochman, Madaline, Wassmer, Mbale, Choi, Seydel, Whitten, Varughese, Grau, Kamiza, Molyneux, Taylor, Lee, Milner and Kim2015). Engagement of human endothelial receptors by infected red blood cells is also known to trigger local signalling processes through angiogenic factors angiopoietin-2 (Ang-2) and vascular endothelial growth factor (VEGF) both of which contribute to or are important drivers of CM pathogenesis (Yeo et al., Reference Yeo, Lampah, Gitawati, Tjitra, Kenangalem, Piera, Price, Duffull, Celermajer and Anstey2008). Thus far, a well-characterized model of human CM remains the P. berghei ANKA strain infection of several mouse strains, specifically the C57BL/6 mouse lineages. In this experimental CM (ECM) model, mice develop similar neurological features to human CM which among others include paralysis, coma and death (Hunt et al., Reference Hunt, Grau, Engwerda, Barnum, van der Heyde, Hansen, Schofield and Golenser2010a). However, some parasitological features of human CM are not apparent in ECM. For instance, sequestration of infected red blood cells does not appear to occur in the P. berghei ECM model. In some observations, parasite sequestration in P. berghei ANKA occurs in the lungs and involves host receptors such CD36 but accumulation in the brain does not correlate with disease pathogenesis (Hearn et al., Reference Hearn, Rayment, Landon, Katz and de Souza2000; Franke-Fayard et al., Reference Franke-Fayard, Janse, Cunha-Rodrigues, Ramesar, Büscher, Que, Löwik, Voshol, den Boer, van Duinen, Febbraio, Mota and Waters2005). This in contrast to other studies which have shown that accumulation of parasitized red blood cells in the brain is necessary for the onset of ECM-related pathology (Amante et al., Reference Amante, Haque, Stanley, Rivera Fde, Randall, Wilson, Yeo, Pieper, Crabb, de Koning-Ward, Lundie, Good, Pinzon-Charry, Pearson, Duke, McManus, Loukas, Hill and Engwerda2010; Baptista et al., Reference Baptista, Pamplona, Pena, Mota, Pied and Vigário2010; Claser et al., Reference Claser, Malleret, Gun, Wong, Chang, Teo, See, Howland, Ginhoux and Rénia2011). More recently, quantitative brain mapping of mice with ECM but infected with a different P. berghei strain (NK65) revealed that parasite-infected red blood cells occluded brain micro-vessels, a feature which was not observed in similar mouse infections with mild disease (Strangward et al., Reference Strangward, Haley, Shaw, Schwartz, Greig, Mironov, de Souza, Cruickshank, Craig, Milner, Allan and Couper2017). In human CM, death is thought to be primarily due to brain swelling depressing the fundus which regulates breathing (Seydel et al., Reference Seydel, Kampondeni, Valim, Potchen, Milner, Muwalo, Birbeck, Bradley, Fox, Glover, Hammond, Heyderman, Chilingulo, Molyneux and Taylor2015), a phenomenon which is yet to be demonstrated in ECM. Even though an increase in brain volume could be the result of immune cell infiltration and parasite sequestration, both of which are also common in ECM, care should be taken in the use of the ECM model to the study of human CM (Craig et al., Reference Craig, Grau, Janse, Kazura, Milner, Barnwell, Turner and Langhorne2012).

P. berghei ECM also appears to be largely an inflammatory syndrome characterized by immune cell infiltration and accumulation of pro-inflammatory cytokines such as IFN-λ and lymphotoxin α (Grau et al., Reference Grau, Heremans, Piguet, Pointaire, Lambert, Billiau and Vassalli1989a, Reference Grau, Tacchini-Cottier, Vesin, Milon, Lou, Piguet and Juillard1993; Engwerda et al., Reference Engwerda, Mynott, Sawhney, De Souza, Bickle and Kaye2002; Ghazanfari et al., Reference Ghazanfari, Mueller and Heath2018). This is relatively divergent from human CM, as despite signs of vascular damage and inflammation in some cases of human CM (Grau et al., Reference Grau, Taylor, Molyneux, Wirima, Vassalli, Hommel and Lambert1989b; Kwiatkowski et al., Reference Kwiatkowski, Hill, Sambou, Twumasi, Castracane, Manogue, Cerami, Brewster and Greenwood1990; Taylor et al., Reference Taylor, Fu, Carr, Whitten, Mueller, Fosiko, Lewallen, Liomba and Molyneux2004), these have been largely refuted as proinflammatory markers appear to poorly associate with human CM in the brains of diseased children (Conroy et al., Reference Conroy, Phiri, Hawkes, Glover, Mallewa, Seydel, Taylor, Molyneux and Kain2010; Erdman et al., Reference Erdman, Dhabangi, Musoke, Conroy, Hawkes, Higgins, Rajwans, Wolofsky, Streiner, Liles, Cserti-Gazdewich and Kain2011). The benefits of the P. berghei ECM model are also challenged by potential intervention approaches that can emerge in such experimental systems. Divergent pathologies between ECM and human CM, be it in cytoadherence biology or immune-based infiltration mechanisms question the utility of the ECM model in evaluating potential inhibitor or adjuvant therapies that are intended for eventual use to treat human CM. Indeed, such interventions, which have relied on or were based on immune mechanisms observed in ECM and to a limited extent, pathological features in some human cases have largely been unsuccessful (Kwiatkowski et al., Reference Kwiatkowski, Molyneux, Stephens, Curtis, Klein, Pointaire, Smit, Allan, Brewster, Grau and Greenwood1993; Prasad and Garner, Reference Prasad and Garner2000; Lell et al., Reference Lell, Köhler, Wamola, Olola, Kivaya, Kokwaro, Wypij, Mithwani, Taylor, Kremsner and Newton2010). Moreover, there appears to be a divergent spectrum in P. berghei ECM phenotypes in different labs, animal strains and P. berghei isolates (Amani et al., Reference Amani, Boubou, Pied, Marussig, Walliker, Mazier and Rénia1998). Standardization of protocols and readouts from such models would thus help in interrogating the important features of ECM and associated interventions and their extrapolation to human CM. More recently, alternatives to the P. berghei ECM model have seen the development and application of humanized SCID mice, into which, human P. falciparum cytoadherence and human CM can be directly modelled. Several humanized mice that can recapitulate human liver and blood-stage malaria disease have been reported, reviewed by Minkah et al. (Reference Minkah, Schafer and Kappe2018). Some early work using some of these mice (engrafted with human red blood cells) has however, demonstrated that P. falciparum infections in these models do not cytoadhere nor lead to CM (Angulo-Barturen et al., Reference Angulo-Barturen, Jiménez-Díaz, Mulet, Rullas, Herreros, Ferrer, Jiménez, Mendoza, Regadera, Rosenthal, Bathurst, Pompliano, Gómez de las Heras and Gargallo-Viola2008). Nevertheless, more recent work, using similar models, in which human vasculature was implanted and allowed to anastomose locally into the host circulatory system has demonstrated a level of in vivo P. falciparum cytoadhesion that will hopefully be useful and refined further to model this aspect of human CM (Meehan et al., Reference Meehan, Scales, Osii, De Niz, Lawton, Marti, Garside, Craig and Brewer2020) leading to potential interventions.

Due to their close relatedness to humans, NHPs have often been promoted as potential powerful alternatives to modelling human CM. NHPs infections with P. coatneyi, a simian malaria parasite, phenotypically resemble the vital aspects of P. falciparum induced human CM such as parasite rosetting, sequestration and the associated pathological features (Udomsangpetch et al., Reference Udomsangpetch, Brown, Smith and Webster1991; Kawai et al., Reference Kawai, Kano and Suzuki1995). Similarly, infections of macaques with P. knowlesi results in severe disease that is lethal to the host within days with a partial sequestration of infected red blood cells in various tissues (Singh and Daneshvar, Reference Singh and Daneshvar2013). Unlike P. berghei which lacks the var gene repertoires that encode for PfEMP-1 in P. falciparum, both P. coatneyi and P. knowlesi possess var like multigene families (SICAvar) which seemingly mediate parasite adhesion properties and antigenic variations (al-Khedery et al., Reference al-Khedery, Barnwell and Galinski1999; Chien et al., Reference Chien, Pakala, Geraldo, Lapp, Humphrey, Barnwell, Kissinger and Galinski2016). Thus, NHPs would offer better models of human CM as better tools to study the neurological aspects of CM such as advanced imaging technologies like MRIs which are revealing important aspects of this disease in humans (Seydel et al., Reference Seydel, Kampondeni, Valim, Potchen, Milner, Muwalo, Birbeck, Bradley, Fox, Glover, Hammond, Heyderman, Chilingulo, Molyneux and Taylor2015) could easily be applied to NHPs. However, this is unlikely as research in these models has been limited by lack of investment and the growing campaigns in the scientific community to entirely abandon the use of NHPs in biomedical research.

Liver stage biology, blood-stage immunity and vaccine development

Animal models of malaria liver stages

Successful transmission of malaria parasites to mosquito vectors (Fig. 1) require inoculation of sporozoites into a mammalian host to initiate a pre-erythrocytic stage in the liver. Unlike blood stages, liver-stage malaria parasites are usually asymptomatic and are often very difficult to produce in vitro. Furthermore, there are the obvious ethical infeasibilities of using the human liver to study such stages in vivo. Thus, RMPs, P. berghei and P. yoelii, have traditionally been used to probe malaria liver stage biology (Ménard et al., Reference Ménard, Tavares, Cockburn, Markus, Zavala and Amino2013). They have been extensively utilized, not just to study liver disease progression, but also the resulting host immunity. Indeed, some of the early seminal work demonstrated that vaccine challenge of mice with irradiated P. berghei sporozoites induced protective immunity to subsequent parasite challenges (Nussenzweig et al., Reference Nussenzweig, Vanderberg, Most and Orton1967). These early studies have been successfully progressed with the current ability to general sporozoite-based vaccine candidates through knockout of specific genes that are conserved in human-infectious Plasmodium or live inoculation with infectious parasites. These approaches elicit protective immune responses by exposing the host to antigens from parasites with arrested development in the liver or through treatment of blood-stage infection upon live sporozoite challenges, reviewed by Goh et al. (Reference Goh, McGuire and Rénia2019). Further to that, both of these parasites have been used to demonstrate the role of humoral and T-cell immunological responses to liver stages of malaria parasites. In P. yoelii, earlier work on monoclonal antibodies raised against a circumsporozoite (CSP) protein were shown to provide immune protection to mice by blocking sporozoite-mediated invasion of hepatocytes (Charoenvit et al., Reference Charoenvit, Mellouk, Cole, Bechara, Leef, Sedegah, Yuan, Robey, Beaudoin and Hoffman1991). Recently, it has been further demonstrated that immunization of mice with late-stage arresting sporozoites that lack a type II fatty acid synthesis enzyme that has been genetically ablated (Pyfabb/f−) result in robust humoral as well as CD4 T-cells immune responses capable of blocking follow-up challenges with wild-type sporozoites (Vaughan et al., Reference Vaughan, O'Neill, Tarun, Camargo, Phuong, Aly, Cowman and Kappe2009; Butler et al., Reference Butler, Schmidt, Vaughan, Aly, Kappe and Harty2011; Keitany et al., Reference Keitany, Sack, Smithers, Chen, Jang, Sebastian, Gupta, Sather, Vignali, Vaughan, Kappe and Wang2014). Similarly, vaccine challenges with a monoclonal antibody (IG1, k) against CSP have been shown to confer protection to mice exposed to otherwise lethal inocula of P. berghei parasites (Potocnjak et al., Reference Potocnjak, Yoshida, Nussenzweig and Nussenzweig1980). Despite the remarkable utility of these rodent RMPs in studying liver stages, significant differences and evolutionary divergences between RMPs and HIPs (Fig. 2) as well as their hosts means biological implications from such models must be very carefully extrapolated. For instance, P. berghei sporozoites can transform into infectious merozoites completing the extraerythrocytic cycle in skin fibroblasts at the site of inoculation of mice without requiring a hepatic cycle (Gueirard et al., Reference Gueirard, Tavares, Thiberge, Bernex, Ishino, Milon, Franke-Fayard, Janse, Ménard and Amino2010). This phenomenon also occurs in P. yoelii but no blood-stage infection ensues (Voza et al., Reference Voza, Miller, Kappe and Sinnis2012). Moreover, differences in duration of liver-stage cycle between human and RMPs (Table 1) as well as the inability of P. berghei and P. yoelli to form hypnozoites (persistent liver stages) further alludes to the complications of using such models to broadly inform on the liver stage biology of all HIPs. Thus far, P. cynomolgi remains the only robust NHP malaria parasite that is extensively used to study P. vivax liver stage biology due to their close relatedness (Fig. 2) (Pasini et al., Reference Pasini, Böhme, Rutledge, Voorberg-Van der Wel, Sanders, Berriman, Kocken and Otto2017) and experimental tractability (Zeeman and Kocken, Reference Zeeman and Kocken2017). The recent adaptation of P. cynomolgi to a robust in vitro culture system (Chua et al., Reference Chua, Ong, Malleret, Suwanarusk, Kosaisavee, Zeeman, Cooper, Tan, Zhang, Tan, Abas, Yip, Elliot, Joyner, Cho, Breyer, Baran, Lange, Maher, Nosten, Bodenreider, Yeung, Mazier, Galinski, Dereuddre-Bosquet, Le Grand, Kocken, Rénia, Kyle, Diagana, Snounou, Russell and Bifani2019b) and the development of human and simian derived hepatocyte organoids which can support ex-vivo propagation of both P. cynomolgi and P. vivax (Chua et al., Reference Chua, Ananthanarayanan, Ong, Wong, Yip, Singh, Qu, Dembele, McMillian, Ubalee, Davidson, Tungtaeng, Imerbsin, Gupta, Andolina, Lee, S-W Tan, Nosten, Russell, Lange, Diagana, Rénia, Yeung, Yu and Bifani2019a) will hopefully help in understanding fundamental aspects of these parasites biology (Table 2).

Table 2.

Common applications of animal models of malaria

In the face of some of the above caveats, human liver-stage biology has been continuously studied using functional in vitro assays. These have included exploratory evaluation of inhibitory activities of immune sera raised against sporozoites infecting cultured human hepatocytes (Huhep) (Kaushansky et al., Reference Kaushansky, Rezakhani, Mann and Kappe2012; Seder et al., Reference Seder, Chang, Enama, Zephir, Sarwar, Gordon, Holman, James, Billingsley, Gunasekera, Richman, Chakravarty, Manoj, Velmurugan, Li, Ruben, Li, Eappen, Stafford, Plummer, Hendel, Novik, Costner, Mendoza, Saunders, Nason, Richardson, Murphy, Davidson, Richie, Sedegah, Sutamihardja, Fahle, Lyke, Laurens, Roederer, Tewari, Epstein, Sim, Ledgerwood, Graham and Hoffman2013). However, the lack of robustness in these assays and the absence of the complex three-dimensional architecture of the ideal liver microenvironment always limit their physiological relevance. The recent development of humanized mice has provided promising models which can indeed capture human liver-stage biology, to extents, which have thus far been unexplorable (Minkah et al., Reference Minkah, Schafer and Kappe2018). Human liver chimaeric mice are currently available to examine the biology of sporozoite invasion of hepatocytes (Vaughan et al., Reference Vaughan, Mikolajczak, Wilson, Grompe, Kaushansky, Camargo, Bial, Ploss and Kappe2012; Mikolajczak et al., Reference Mikolajczak, Vaughan, Kangwanrangsan, Roobsoong, Fishbaugher, Yimamnuaychok, Rezakhani, Lakshmanan, Singh, Kaushansky, Camargo, Baldwin, Lindner, Adams, Sattabongkot and Kappe2015). In these mice, huHep are engrafted under severe combined immunodeficiency (SCID) followed by depletion of host hepatocytes to allow for propagation of huHep in mice liver parenchyma. huHep mice models on SCID background have demonstrated successful infection with P. falciparum sporozoites that develop into liver-stage schizonts which in turn release exo-erythrocytic merozoites (Morosan et al., Reference Morosan, Hez-Deroubaix, Lunel, Renia, Giannini, Van Rooijen, Battaglia, Blanc, Eling, Sauerwein, Hannoun, Belghiti, Brechot, Kremsdorf and Druilhe2006; Sacci et al., Reference Sacci, Alam, Douglas, Lewis, Tyrrell, Azad and Kneteman2006). These humanized huHep mice have also been used to explore the role of human immune responses to liver stages of malaria parasites. Passive immunization of huHep mice with monoclonal antibodies raised against P. falciparum sporozoites has been shown to block the establishment of liver-stage infection (Foquet et al., Reference Foquet, Hermsen, van Gemert, Van Braeckel, Weening, Sauerwein, Meuleman and Leroux-Roels2014). Mice transplanted with human immune system components (CD4, CD8 or B cells) have also been developed and used to characterize equivalent human immune responses to liver stages of malaria parasites. These mice were produced in immunocompromised backgrounds by adenoviral transduction of human HLA class II alleles followed by engraftment with haematopoietic CD34+ cells, which can proliferate to different immune cell subsets. Immunization of these mice with P. falciparum CSP provided protection to transgenic P. berghei infections carrying P. falciparum CSP (Huang et al., Reference Huang, Li, Coelho-dos-Reis, Zhang, Mitchell, Nogueira, Tsao, Noe, Ayala, Sahi, Gutierrez, Nussenzweig, Wilson, Nardin, Nussenzweig and Tsuji2015). Nevertheless, the current generation of humanized mice lack adequate tissue penetration of engrafted cells while the requirement for the use of SCID conditions to maintain such cells in the host limits their use in probing certain aspects of parasite biology. Whilst they remain highly artificial, the evolution and further refinement of these models is, however, opening new exciting avenues into not just the in vivo liver stage biology of malaria parasites, but other stages as well (Minkah et al., Reference Minkah, Schafer and Kappe2018).

Efficacy models of antimalarial drug action and resistance

In antimalarial drug discovery programmes, animal models of malaria are widely used to evaluate in vivo efficacy and physiological context of the drugs before human phase clinical trials (Fidock et al., Reference Fidock, Rosenthal, Croft, Brun and Nwaka2004). These pre-clinical evaluations allow for deconvolution of in vivo drug potency, pharmacodynamics/pharmacokinetics (absorption, metabolism, distribution and excretion; ADME) and toxicities. Such profiles fine tune the discovery pipeline by selecting antimalarial agents with better potency and safety landscapes in a hit to lead optimization strategies. Animals have also been used to decipher the genetic basis of antimalarial drug resistance through in vivo drug selection and more recently to validate some in vivo phenotypes of orthologous drug resistance markers identified in P. falciparum.

Hit to lead optimization of antimalarial drug candidates

Antimalarial drug discovery programmes are mostly based on in vitro whole cell phenotypic screens of Plasmodium parasites within host red cells (Guiguemde et al., Reference Guiguemde, Shelat, Bouck, Duffy, Crowther, Davis, Smithson, Connelly, Clark, Zhu, Jiménez-Díaz, Martinez, Wilson, Tripathi, Gut, Sharlow, Bathurst, El Mazouni, Fowble, Forquer, McGinley, Castro, Angulo-Barturen, Ferrer, Rosenthal, Derisi, Sullivan, Lazo, Roos, Riscoe, Phillips, Rathod, Van Voorhis, Avery and Guy2010; Chatterjee and Yeung, Reference Chatterjee and Yeung2012) even though target-based screens (utilizing recombinant P. falciparum proteins) have become an option recently (Phillips et al., Reference Phillips, Lotharius, Marsh, White, Dayan, White, Njoroge, El Mazouni, Lao, Kokkonda, Tomchick, Deng, Laird, Bhatia, March, Ng, Fidock, Wittlin, Lafuente-Monasterio, Benito, Alonso, Martinez, Jimenez-Diaz, Bazaga, Angulo-Barturen, Haselden, Louttit, Cui, Sridhar, Zeeman, Kocken, Sauerwein, Dechering, Avery, Duffy, Delves, Sinden, Ruecker, Wickham, Rochford, Gahagen, Iyer, Riccio, Mirsalis, Bathhurst, Rueckle, Ding, Campo, Leroy, Rogers, Rathod, Burrows and Charman2015; Alam et al., Reference Alam, Sanchez-Azqueta, Janha, Flannery, Mahindra, Mapesa, Char, Sriranganadane, Brancucci, Antonova-Koch, Crouch, Simwela, Millar, Akinwale, Mitcheson, Solyakov, Dudek, Jones, Zapatero, Doerig, Nwakanma, Vázquez, Colmenarejo, Lafuente-Monasterio, Leon, Godoi, Elkins, Waters, Jamieson, Álvaro, Ranford-Cartwright, Marti, Winzeler, Gamo and Tobin2019). Phenotypic screens yield hundred to thousands of chemical scaffolds which are prioritized based on in vitro antimalarial activity and in silico-predicted physicochemical properties (ADME). Scaffolds with better profiles in the above assays are further refined to achieve better antimalarial potency or improve their ADME and toxicity safety scores. New scaffolds which pass the established benchmarks are then tested for in vivo efficacy and safety, usually in a small animal model. These in vivo proofs of concept studies often utilize RMPs, particularly P. berghei and P. yoelii (Fidock et al., Reference Fidock, Rosenthal, Croft, Brun and Nwaka2004). P. berghei remains the most commonly used RMP for this purpose (Fidock et al., Reference Fidock, Rosenthal, Croft, Brun and Nwaka2004). However, the choice of rodent parasite spp. can also depend on the antimalarial drug candidates under evaluation or the drug targets under investigation. For instance, pyridones, compounds targeting the cytochrome bc1 complex, have been evaluated in P. yoelii because of the close genetic similarity of this target protein between P. yoelii and P. falciparum as opposed to the slightly divergent P. berghei (Yeates et al., Reference Yeates, Batchelor, Capon, Cheesman, Fry, Hudson, Pudney, Trimming, Woolven, Bueno, Chicharro, Fernández, Fiandor, Gargallo-Viola, Gómez de las Heras, Herreros and León2008). Moreover, P. berghei is inherently less susceptible to some classes of endoperoxides (Lee et al., Reference Lee, Waters and Brewer2018; Simwela et al., Reference Simwela, Hughes, Roberts, Rennie, Barrett and Waters2020a, Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b) while P. yoelii is naturally resistant to quinolines (Warhurst and Killick-Kendrick, Reference Warhurst and Killick-Kendrick1967). Some of the differences in drug susceptibility between RMPs (P. berghei, P. yoelii) and P. falciparum could be due to reticulocyte preferences for the former which provide rich metabolic energy sources with the potential to cushion the killing effect of antimalarial agents (Srivastava et al., Reference Srivastava, Creek, Evans, De Souza, Schofield, Müller, Barrett, McConville and Waters2015). Care should, therefore, be taken when using these models for evaluating different classes of antimalarial agents, particularly metabolism-based inhibitors. The most widely used initial screen in these RMPs is the Peter's 4 day suppressive test (Peters and Robinson, Reference Peters, Robinson, Zak and Sande1999a). In this test, mice are infected with fixed parasite inocula and dosed with the drug (through appropriate channels) a few hours post-infection for four consecutive days. Parasitaemia in treated mice is then compared to untreated controls on day four post infection from which percentage suppression is usually calculated in further reference to a known antimalarial agent with proven and quantified activity. Compound series which achieve superior suppression in the four-day suppressive test are then further tested in follow up assays such as dose-escalation studies to determine the 50 and 90% effective (i.e. parasite death) doses (ED50, ED90). Further assessments of in vivo drug potency, bioavailability, toxicity and mode of delivery are also carried out (Fidock et al., Reference Fidock, Rosenthal, Croft, Brun and Nwaka2004). Other tests may include recrudescence assays where candidate antimalarial agents are evaluated on their ability to suppress parasites for a specific duration of time post-treatment and prophylaxis potential where compounds are administered first before infection and their preventive potential assessed in daily follow-ups. Compound series that perform best in the above benchmarks are either expanded for further lead optimization or progressed through candidate selection filters before embarking on clinical development programmes. In either case, RMPs are used in evaluating further leads, re-optimizing expanded leads and or evaluating their overall potency (Fig. 3). RMPs can also be used to assess in vitro potency of antimalarial agents in short-term maturation assays (Franke-Fayard et al., Reference Franke-Fayard, Djokovic, Dooren, Ramesar, Waters, Falade, Kranendonk, Martinelli, Cravo and Janse2008). This can provide necessary bridging information to explain potential discrepancies between in vitro (P. falciparum) and in vivo (P. berghei) sensitivities for some inhibitors and or whether such discrepancies are due to intrinsic differences between the parasite species or due to the pharmacodynamic/pharmacokinetic properties of the drug in the animal model. Since proof of concept in an animal model is usually required before any drug discovery programme is progressed, RMPs have, indeed, been at the front of these evaluations as most antimalarial drug candidates in clinical development at the moment (KAF156, KAE609, OZ349, DDD107498) were all shown to cure mice infected with P. berghei (Rottmann et al., Reference Rottmann, McNamara, Yeung, Lee, Zou, Russell, Seitz, Plouffe, Dharia, Tan, Cohen, Spencer, González-Páez, Lakshminarayana, Goh, Suwanarusk, Jegla, Schmitt, Beck, Brun, Nosten, Renia, Dartois, Keller, Fidock, Winzeler and Diagana2010; Charman et al., Reference Charman, Arbe-Barnes, Bathurst, Brun, Campbell, Charman, Chiu, Chollet, Craft, Creek, Dong, Matile, Maurer, Morizzi, Nguyen, Papastogiannidis, Scheurer, Shackleford, Sriraghavan, Stingelin, Tang, Urwyler, Wang, White, Wittlin, Zhou and Vennerstrom2011; Kuhen et al., Reference Kuhen, Chatterjee, Rottmann, Gagaring, Borboa, Buenviaje, Chen, Francek, Wu, Nagle, Barnes, Plouffe, Lee, Fidock, Graumans, van de Vegte-Bolmer, van Gemert, Wirjanata, Sebayang, Marfurt, Russell, Suwanarusk, Price, Nosten, Tungtaeng, Gettayacamin, Sattabongkot, Taylor, Walker, Tully, Patra, Flannery, Vinetz, Renia, Sauerwein, Winzeler, Glynne and Diagana2014; Baragaña et al., Reference Baragaña, Hallyburton, Lee, Norcross, Grimaldi, Otto, Proto, Blagborough, Meister, Wirjanata, Ruecker, Upton, Abraham, Almeida, Pradhan, Porzelle, Luksch, Martínez, Luksch, Bolscher, Woodland, Norval, Zuccotto, Thomas, Simeons, Stojanovski, Osuna-Cabello, Brock, Churcher, Sala, Zakutansky, Jiménez-Díaz, Sanz, Riley, Basak, Campbell, Avery, Sauerwein, Dechering, Noviyanti, Campo, Frearson, Angulo-Barturen, Ferrer-Bazaga, Gamo, Wyatt, Leroy, Siegl, Delves, Kyle, Wittlin, Marfurt, Price, Sinden, Winzeler, Charman, Bebrevska, Gray, Campbell, Fairlamb, Willis, Rayner, Fidock, Read and Gilbert2015). Recently, drug discovery programmes are also incorporating humanized mice infected with human P. falciparum in evaluating the in vivo efficacy of antimalarial drug candidates in addition to the traditional RMPs (Coslédan et al., Reference Coslédan, Fraisse, Pellet, Guillou, Mordmüller, Kremsner, Moreno, Mazier, Maffrand and Meunier2008; Booker et al., Reference Booker, Bastos, Kramer, Barker, Skerlj, Sidhu, Deng, Celatka, Cortese, Guerrero Bravo, Crespo Llado, Serrano, Angulo-Barturen, Jiménez-Díaz, Viera, Garuti, Wittlin, Papastogiannidis, Lin, Janse, Khan, Duraisingh, Coleman, Goldsmith, Phillips, Munoz, Wirth, Klinger, Wiegand and Sybertz2010; Barker et al., Reference Barker, Urgaonkar, Mazitschek, Celatka, Skerlj, Cortese, Tyndall, Liu, Cromwell, Sidhu, Guerrero-Bravo, Crespo-Llado, Serrano, Lin, Janse, Khan, Duraisingh, Coleman, Angulo-Barturen, Jiménez-Díaz, Magán, Gomez, Ferrer, Martínez, Wittlin, Papastogiannidis, O'Shea, Klinger, Bree, Lee, Levine, Wiegand, Munoz, Wirth, Clardy, Bathurst and Sybertz2011; Nilsen et al., Reference Nilsen, LaCrue, White, Forquer, Cross, Marfurt, Mather, Delves, Shackleford, Saenz, Morrisey, Steuten, Mutka, Li, Wirjanata, Ryan, Duffy, Kelly, Sebayang, Zeeman, Noviyanti, Sinden, Kocken, Price, Avery, Angulo-Barturen, Jiménez-Díaz, Ferrer, Herreros, Sanz, Gamo, Bathurst, Burrows, Siegl, Guy, Winter, Vaidya, Charman, Kyle, Manetsch and Riscoe2013; Baragaña et al., Reference Baragaña, Hallyburton, Lee, Norcross, Grimaldi, Otto, Proto, Blagborough, Meister, Wirjanata, Ruecker, Upton, Abraham, Almeida, Pradhan, Porzelle, Luksch, Martínez, Luksch, Bolscher, Woodland, Norval, Zuccotto, Thomas, Simeons, Stojanovski, Osuna-Cabello, Brock, Churcher, Sala, Zakutansky, Jiménez-Díaz, Sanz, Riley, Basak, Campbell, Avery, Sauerwein, Dechering, Noviyanti, Campo, Frearson, Angulo-Barturen, Ferrer-Bazaga, Gamo, Wyatt, Leroy, Siegl, Delves, Kyle, Wittlin, Marfurt, Price, Sinden, Winzeler, Charman, Bebrevska, Gray, Campbell, Fairlamb, Willis, Rayner, Fidock, Read and Gilbert2015). NHPs have also been used to evaluate the in vivo efficacy of antimalarial drug candidates, but they are at present mostly restricted to the evaluation of agents that are required for radical cure of chronic infections caused by P. vivax using its surrogate model, P. cynomolgi (Zeeman and Kocken, Reference Zeeman and Kocken2017).

Fig. 3.

A simplified flow chart of the antimalarial drug discovery pipeline showing the utility of animal models. Discovery programmes usually start with in vitro whole cell phenotypic screens. Compounds to be progressed are selected based on the established half-inhibitory concentrations (IC₅₀) cut-off values. These benchmarks vary between different programmes but usually compounds which achieve a <1 μ m IC₅₀ are preferred. Selected hits are either chemically refined, expanded and or profiled for pharmacodynamics (PD) and pharmacokinetics (PK) profiles in silico and in situ. Refined hits are re-evaluated for their potency in vitro against P. falciparum and later in vivo in selected animal models. In vivo evaluations may include PD/PK analysis, suppressive test, dose ascendency and recrudescence assays. Based on established benchmarks, lead compounds are progressed to human trials. During hit selection, several approaches may be used to identify the compound molecular and biochemical targets. These may include selection for resistance and forward genetic screening, proteomics and metabolomics. Target pathways are then validated using reverse genetics approaches by CRISPR-Cas9 or other gene knockout/knockdown approaches. In certain instances, compounds can be progressed without knowledge of the drug target. In these cases resistance can be identified in field isolates and the mutations retrospectively mapped to identify the drug targets and mode of resistance. Stages where animal models are often used are highlighted in light green.

Mode of action studies and genetic basis of drug resistance

The utility of RMPs in understanding the genetic basis of drug resistance has also been exploited (Carlton et al., Reference Carlton, Hayton, Cravo and Walliker2001). Not only have murine malaria parasites been used to confirm some of the drug resistance mutations observed in P. falciparum (Fig. 3), some resistance mutation alleles first identified in P. falciparum are now routinely used as selection markers for transfection experiments across the parasite spp. (van Dijk et al., Reference van Dijk, Waters and Janse1995; Carlton et al., Reference Carlton, Vinkenoog, Waters and Walliker1998b, Reference Carlton, Hayton, Cravo and Walliker2001). Another advantage of RMPs is often the ease with which drug resistance can be selected. In P. falciparum forward genetics approaches, selection for drug resistance can be a long and tedious process which can take from a few weeks to years. For example, in vitro selection for resistance to artemisinin in P. falciparum took almost 4–5 years to obtain stable resistant parasites (Witkowski et al., Reference Witkowski, Lelièvre, Barragán, Laurent, Su, Berry and Benoit-Vical2010; Demas et al., Reference Demas, Sharma, Wong, Early, Redmond, Bopp, Neafsey, Volkman, Hartl and Wirth2018). On the contrary, drug resistance in RMPs, P. berghei and P. chabaudi can be selected within a short period of time. Resistance to GNF179, a related compound to KAF156 was selected after just 2 single in vivo dose treatments in P. berghei (Lim et al., Reference Lim, LaMonte, Lee, Reimer, Tan, Corey, Tjahjadi, Chua, Nachon, Wintjens, Gedeck, Malleret, Renia, Bonamy, Ho, Yeung, Chow, Lim, Fidock, Diagana, Winzeler and Bifani2016), something which took up to 4 months in P. falciparum (Kuhen et al., Reference Kuhen, Chatterjee, Rottmann, Gagaring, Borboa, Buenviaje, Chen, Francek, Wu, Nagle, Barnes, Plouffe, Lee, Fidock, Graumans, van de Vegte-Bolmer, van Gemert, Wirjanata, Sebayang, Marfurt, Russell, Suwanarusk, Price, Nosten, Tungtaeng, Gettayacamin, Sattabongkot, Taylor, Walker, Tully, Patra, Flannery, Vinetz, Renia, Sauerwein, Winzeler, Glynne and Diagana2014). In P. chabaudi, resistance to pyrimethamine was obtained within 2 weeks after a single dose treatment (Carter and Walliker, Reference Carter and Walliker1975). From these pyrimethamine resistant P. chabaudi lines, additional lines resistant to ascending doses of chloroquine, mefloquine, artemisinin and artesunate have been easily derived (Rosario, Reference Rosario1976; Padua, Reference Padua1981; Carlton et al., Reference Carlton, Mackinnon and Walliker1998a; Cravo et al., Reference Cravo, Carlton, Hunt, Bisoni, Padua and Walliker2003; Afonso et al., Reference Afonso, Hunt, Cheesman, Alves, Cunha, do Rosário and Cravo2006). Unlike in P. falciparum, drug resistance in rodent malarias can also be tested for in vivo phenotype stability in the absence of drug pressure through blood passage, freeze–thaw cycles and the mosquito infectivity and transmission filters (Rosario, Reference Rosario1976; Afonso et al., Reference Afonso, Hunt, Cheesman, Alves, Cunha, do Rosário and Cravo2006). After obtaining drug-resistant parasites, genetic markers responsible for these phenotypes have been characterized by carrying out genetic crosses between sensitive parasites and resistant clones. This typically involves the transmission of sensitive and resistant parasites in a mixture into a mosquito then into a new host which allows for the selection of recombinant progenies from which chromosomal linkage analysis can be used to map candidate genes to the observed phenotypes. Even though this is also possible in P. falciparum (which may require NHPs or adapted humanized mouse models), RMPs are uniquely suited for such endeavours due to the ease of handling rodents and the ability to reproduce the entire in vivo life cycle under lab conditions (Carlton et al., Reference Carlton, Hayton, Cravo and Walliker2001). In the meantime, the advent of recent genome sequencing technologies means candidate drug-resistant mutations in these rodent models can be quickly identified and characterized (Hunt et al., Reference Hunt, Afonso, Creasey, Culleton, Sidhu, Logan, Valderramos, McNae, Cheesman, do Rosario, Carter, Fidock and Cravo2007, Reference Hunt, Martinelli, Modrzynska, Borges, Creasey, Rodrigues, Beraldi, Loewe, Fawcett, Kumar, Thomson, Trivedi, Otto, Pain, Blaxter and Cravo2010b; Borges et al., Reference Borges, Cravo, Creasey, Fawcett, Modrzynska, Rodrigues, Martinelli and Hunt2011; Kinga Modrzynska et al., Reference Kinga Modrzynska, Creasey, Loewe, Cezard, Trindade Borges, Martinelli, Rodrigues, Cravo, Blaxter, Carter and Hunt2012). A brief role of RMPs in understanding the mode of action and resistance for principle antimalarial drugs that are and have been in clinical usage is described in detail in the following sections.

Sulphadoxine and pyrimethamine

Resistance to antifolates is perhaps one of the well-studied and characterized resistance mechanisms in malaria parasites. Parasite resistance to antifolates is thought to occur by an initial amplification of the target locus followed by more rapid mutations that the multigenic nature of the locus facilitates which with continued selection pressure fixates into a single locus through maintenance and propagation of favourable mutations in the population (Tanaka et al., Reference Tanaka, Gu, Bzik, Li and Inselburg1990). This also appears to be a common mechanism to early drug resistance in most eukaryotic pathogens where transport and drug efflux genes are amplified through copy number duplications before acquisition of target-specific mutations (Fairlamb et al., Reference Fairlamb, Gow, Matthews and Waters2016). Meanwhile, resistance to sulphadoxine and pyrimethamine (SP) emerged immediately after this drug combination was rolled out for clinical use. The mechanistic details of resistance to these two drugs have now been well described (Plowe et al., Reference Plowe, Cortese, Djimde, Nwanyanwu, Watkins, Winstanley, Estrada-Franco, Mollinedo, Avila, Cespedes, Carter and Doumbo1997). The earliest report of an RMP resistant to pyrimethamine was in 1952 where a P. berghei strain with up to 20-fold resistance as compared to the wild type was obtained after two rounds of passages and treatment with single curative doses (Rollo, Reference Rollo1952). Several other P. berghei parasites resistant to pyrimethamine have also been easily obtained and reported (Diggens, Reference Diggens1970; van Dijk et al., Reference van Dijk, McConkey, Vinkenoog, Waters and Janse1994). Pyrimethamine resistance has also been selected for in the other RMPs (Yoeli et al., Reference Yoeli, Upmanis and Most1969; Walliker et al., Reference Walliker, Carter and Morgan1973, Reference Walliker, Carter and Sanderson1975). However, the mechanism of pyrimethamine resistance in these lines was not convincingly known until mutations in the dhfr gene, specifically the S108N substitution, was identified in P. falciparum after a genetic cross of pyrimethamine-resistant field isolates with laboratory-sensitive lines (Cowman et al., Reference Cowman, Morry, Biggs, Cross and Foote1988; Peterson et al., Reference Peterson, Walliker and Wellems1988). In these crosses, resistant parasites consistently inherited a fragment within the dhfr which differed from sensitive parasites by either the S108N substitutions or other candidate mutations such as N51I or C59R which are now all validated determinants of pyrimethamine resistance. Crucially, equivalent mutations in the dhfr such as the S106N were later identified in the P. chabaudi pyrimethamine resistant line (AS-Pyr) (Cheng and Saul, Reference Cheng and Saul1994). A similar mutation (S110N) is also responsible for the dhfr-mediated pyrimethamine resistance phenotype in P. berghei (van Dijk et al., Reference van Dijk, McConkey, Vinkenoog, Waters and Janse1994). Mutant dhfr coupled to thymidylate synthase (dhfr/ts) carrying pyrimethamine resistance alleles are currently a widely used drug selection marker for transfection experiments in both P. berghei and P. falciparum (van Dijk et al., Reference van Dijk, Waters and Janse1995; Wu et al., Reference Wu, Kirkman and Wellems1996) as well as P. knowlesi (van der Wel et al., Reference van der Wel, Tomás, Kocken, Malhotra, Janse, Waters and Thomas1997; Mohring et al., Reference Mohring, Hart, Rawlinson, Henrici, Charleston, Diez Benavente, Patel, Hall, Almond, Campino, Clark, Sutherland, Baker, Draper and Moon2019). Even though mutations in the dhps gene are predicted determinants of resistance to sulphadoxine (Plowe et al., Reference Plowe, Cortese, Djimde, Nwanyanwu, Watkins, Winstanley, Estrada-Franco, Mollinedo, Avila, Cespedes, Carter and Doumbo1997), this remains circumstantial due to a lack of in vitro assays that can reliably distinguish sulphadoxine resistant from sensitive parasites (Wang et al., Reference Wang, Sims and Hyde1997). Sulphadoxine is a sulphonamide that acts as a substrate analogue of p-aminobenzoic acid (PABA) to competitively inhibit dhps which in turn affects downstream folate synthesis for the parasite. Due to the variations in the levels of PABA in most culture media, phenotyping of resistance levels to sulphadoxine has been particularly difficult (Watkins et al., Reference Watkins, Sixsmith, Chulay and Spencer1985; Wang et al., Reference Wang, Sims and Hyde1997). Nevertheless, transfection and allelic exchange experiments have been used to validate some of dhps alleles such as the A437G substitution in modulating in vitro susceptibility to this drug (Triglia et al., Reference Triglia, Wang, Sims, Hyde and Cowman1998). Due to these complexities, the genetics of dual resistance to SP drug combinations have been difficult to unravel. Parasites exhibiting SP resistance can carry mutations in the dhfr and dhps genes even though dhfr gene mutations alone are known to mediate resistance phenotypes to both drugs while dhps polymorphisms can sometimes less clearly correlate with SP resistance (Plowe et al., Reference Plowe, Cortese, Djimde, Nwanyanwu, Watkins, Winstanley, Estrada-Franco, Mollinedo, Avila, Cespedes, Carter and Doumbo1997). RMPs can, therefore, in these situations offer a unique opportunity for studying resistant phenotypes emanating from such drug combinations as levels of interfering parameters such as PABA can be controlled, physiologically or through artificial diet supplementation. Parasites resistant to sulphadoxine have been selected in both P. berghei and P. chabaudi, both of which appear to need less PABA as they develop an increased capacity to synthesize this metabolite de novo (Singh et al., Reference Singh, Ramakrishnan, Prakash and Bhatnagar1954; Carlton et al., Reference Carlton, Hayton, Cravo and Walliker2001). However, the genetic determinants in these resistant lines have remained uncharacterized. Crucially, P. berghei parasites resistant to SP drug combinations have been successfully obtained using a continuous low dose selection strategy even though the resistant phenotypes were unstable and the genetic determinants have not been identified (Merkli and Richle, Reference Merkli and Richle1983b). Perhaps one of the best-characterized SP-resistant RMP line is the P. chabaudi AS (50S/P) line. This line was obtained by a further selection of the AS-Pyr line with a single four-day high dose exposure with the SP drug combination to obtain parasite progenies that were strongly resistant to the drug combination. However, quantitative trait loci and genetic analysis of the AS (50S/P) line revealed that dhfr mutations were the major determinant of the SP drug resistance phenotype as no additional dhps mutations were identified (Hayton et al., Reference Hayton, Ranford-Cartwright and Walliker2002).

Artemisinin

Artemisinins (ARTs) are frontline antimalarial drugs in ART-based combination therapies, their deployment of which has played significant roles in alleviating the global malaria disease burden (WHO, 2020). However, resistance to ARTs has emerged and is now endemic in most parts of SEA (WHO, 2020). ART resistance is primarily conferred by polymorphisms in a Kelch13 protein (Ariey et al., Reference Ariey, Witkowski, Amaratunga, Beghain, Langlois, Khim, Kim, Duru, Bouchier, Ma, Lim, Leang, Duong, Sreng, Suon, Chuor, Bout, Ménard, Rogers, Genton, Fandeur, Miotto, Ringwald, Le Bras, Berry, Barale, Fairhurst, Benoit-Vical, Mercereau-Puijalon and Ménard2014) even though several other determinants such as UBP-1, Pfcoronin, falcipains and AP2-μ have been implicated (Hunt et al., Reference Hunt, Afonso, Creasey, Culleton, Sidhu, Logan, Valderramos, McNae, Cheesman, do Rosario, Carter, Fidock and Cravo2007; Henriques et al., Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013; Demas et al., Reference Demas, Sharma, Wong, Early, Redmond, Bopp, Neafsey, Volkman, Hartl and Wirth2018; Rocamora et al., Reference Rocamora, Zhu, Liong, Dondorp, Miotto, Mok and Bozdech2018). Meanwhile, RMPs have been instrumental in identifying some determinants of resistance to ARTs. ART resistant P. berghei and P. yoelii parasites were first selected and reported in the late 1990s (Peters and Robinson, Reference Peters, Robinson, Zak and Sande1999a). This involved the application of the 2% relapse technique where parasites are inoculated into mice and treated with a high subcutaneous dose of the drug 3-h post infection. Upon recrudescence, parasites are passaged into a new host and retreated with similar drug doses. Levels of resistance are quantified by graphing the changes in time required to reach 2% parasitaemia in the treatment group which can be graded as a progressive reduction in the time required to reach 2% parasitaemia over the course of the passages when resistance is successfully obtained. Using these approaches, resistance to ARTs was obtained in both P. berghei and P. yoelii which was, however, unstable as resistant parasites of both species easily lost the phenotype when the drug was withdrawn (although the lines were uncloned and overgrowth by wildtype sensitive parasites could have occurred) (Peters and Robinson, Reference Peters and Robinson1999b). Biochemical characterization of one of these ART-resistant P. yoelii strain which displayed up to four-fold resistance compared to the sensitive lines revealed a reduced accumulation of the radiolabelled drug in the resistant parasites (Walker et al., Reference Walker, Pitsch, Peng, Robinson, Peters, Bhisutthibhan and Meshnick2000). Another selection for ART resistance in P. berghei was attempted using the ART derivative artemether in the early 2000s (Xiao et al., Reference Xiao, Yao, Utzinger, Cai, Chollet and Tanner2004). Infected mice were treated with high doses of artemether, passaged into a new host upon recrudescence and retreated every passage for 50 passages. Even though up to 8-fold resistance was achieved in these lines, the phenotype was unstable as drug sensitivity was retained after a few rounds of infections without drug pressure. The most studied RMPs which displayed stable ART resistance phenotypes were obtained in P. chabaudi and were first reported in 2006 (Afonso et al., Reference Afonso, Hunt, Cheesman, Alves, Cunha, do Rosário and Cravo2006). These lines were selected from P. chabaudi clones which had and were already previously selected for resistance to pyrimethamine and chloroquine (Fig. 4). The original P. chabaudi AS isolate was exposed to four consecutive doses of pyrimethamine at 50 mg kg⁻¹ from which a pyrimethamine resistant line (AS-Pyr) was obtained and cloned (Walliker et al., Reference Walliker, Carter and Sanderson1975). The AS-Pyr line was then selected for resistance to chloroquine from which a line resistant to six consecutive doses of the drug at 3 mg kg⁻¹ (AS-3CQ) was obtained (Rosario, Reference Rosario1976). Selection of the AS-3CQ line with a stepwise chloroquine dose increment yielded a P. chabaudi line that was resistant up to six consecutive daily doses of chloroquine at 15 mg kg⁻¹ (AS-15CQ) (Padua, Reference Padua1981). From the AS-15CQ line, several lines with differing drug resistance phenotypes were subsequently obtained. Exposure of the AS-15CQ line to a gradual ascending dose of mefloquine (7–30 mg kg⁻¹) resulted in the parasite line that was initially resistant to up to four consecutive doses of mefloquine at 30 mg kg⁻¹ but eventually lost some degree of resistance by only surviving four consecutive doses of the drug at 15 mg kg⁻¹ (designated AS-15MF) (Cravo et al., Reference Cravo, Carlton, Hunt, Bisoni, Padua and Walliker2003). The AS-15CQ line was also subjected to a further chloroquine selection until a line resistant to up to 30 mg kg⁻¹ of chloroquine (AS-30CQ) was obtained (Padua, Reference Padua1981; Carlton et al., Reference Carlton, Mackinnon and Walliker1998a). Selection of AS-30CQ with gradually increasing doses of ART (up to 300 mg kg⁻¹) yielded an ART-resistant line (AS-ART) that survived three to five consecutive doses (up to 300 mg kg⁻¹) of the drug (Afonso et al., Reference Afonso, Hunt, Cheesman, Alves, Cunha, do Rosário and Cravo2006; Henriques et al., Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013). From the AS-15CQ, another selection with incremental doses of artesunate also yielded an independent line (AS-ATN) that was resistant to artesunate surviving up to 60 mg kg⁻¹ of the drug (Afonso et al., Reference Afonso, Hunt, Cheesman, Alves, Cunha, do Rosário and Cravo2006) (Fig. 4). Interestingly, both the AS-30CQ and AS-ART appear to have shared a cross resistance to the ART phenotype (Henriques et al., Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013). Three independent genetic crosses of the AS-ART line with a parallel P. chabaudi sensitive line and follow-up linkage group selection analysis identified a selection valley on chromosome 2 on the resistant parasites that strongly associated with the ART resistance phenotype. Within this locus, two mutations in a deubiquitinating enzyme, UBP-1 (close human homologue USP7) appear to have fixed independently in the AS-ATN (V2697F), AS-30CQ and AS-ART line (V2728F) (Hunt et al., Reference Hunt, Afonso, Creasey, Culleton, Sidhu, Logan, Valderramos, McNae, Cheesman, do Rosario, Carter, Fidock and Cravo2007). Meanwhile, whole-genome sequencing further revealed that the V2728F mutation was not just common to the AS-30CQ and AS-ART lines, but also in the AS-15MF line (Hunt et al., Reference Hunt, Martinelli, Modrzynska, Borges, Creasey, Rodrigues, Beraldi, Loewe, Fawcett, Kumar, Thomson, Trivedi, Otto, Pain, Blaxter and Cravo2010b). Prior analysis of the AS-Pyr already identified the expected S106N dhfr gene mutation that was chiefly responsible for the pyrimethamine resistance phenotype (Cheng and Saul, Reference Cheng and Saul1994). Further genetic analysis of these lines also revealed several other polymorphisms which may have arose as a consequence of the drug selection cascade from the original AS line. These include a mutation (A173E) in the amino acid transporter (aat, PCHAS_1127800) that seemingly was responsible for the chloroquine resistance phenotype in the AS-3CQ line and another mutation (T719N) in a predicted unknown transporter (PCHAS_0313700) which appears to have led to the emergence of the chloroquine resistance phenotype in the AS-15CQ line (Kinga Modrzynska et al., Reference Kinga Modrzynska, Creasey, Loewe, Cezard, Trindade Borges, Martinelli, Rodrigues, Cravo, Blaxter, Carter and Hunt2012). Nevertheless, it appears that the two UBP-1 mutations may have arose independently in the AS-15CQ uncloned line which resulted in their specific fixation when a drug pressure of mefloquine, artesunate or a higher dose of chloroquine was applied (Henriques et al., Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013). Further analysis of the ART cross-resistance phenotype between the AS-30CQ and AS-ART also revealed that selection of the former line with ART led to the successful acquisition of an additional mutation (I568T) in the AP-2 μ gene which was responsible for the higher level of ART resistance in the AS-ART as compared to the AS-30CQ (Henriques et al., Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013). However, despite the observation of some of these mutations (UBP-1 and AP-2 μ) in P. falciparum clinical isolates that have presented with potential ART resistance phenotypes (Henriques et al., Reference Henriques, Hallett, Beshir, Gadalla, Johnson, Burrow, van Schalkwyk, Sawa, Omar, Clark, Bousema and Sutherland2014), up until recently (discussed below), their role in mediating resistance to these drugs remained an association in part due to the complexity of the selection procedure with multiple drugs as well as the absence of appropriate reverse genetics approaches.

Fig. 4.

Selection strategies used to obtain P. chabaudi artemisinin-resistant lines and the causal genetic determinants. The original AS line was subjected to four daily doses of pyrimethamine to obtain the AS-Pyr resistant line that carry the S106N mutation in the dhfr gene. Further selection of this line with chloroquine (CQ) resulted in the AS-3CQ resistant line that was able to tolerate up to six consecutive doses of CQ at 3 mg kg⁻¹. Whole-genome sequencing identified the A173R mutation in an amino acid transporter (aat) to be responsible for this phenotype. Further selection of this line with incremental doses of CQ resulted in the AS-15CQ line which carried two UBP-1 mutations, V2697F and V2728F. From this line, incremental dose selection with mefloquine, artesunate and further high doses of CQ yielded the AS-15MF, AS-ATN and AS-30CQ which appear to have fixated the UBP-1 mutations differently as indicated. Selection of the AS-30CQ line with ART resulted in the AS-ART line which carries an additional mutation in the AP-2 μ gene. Adapted from Hunt et al. (Reference Hunt, Martinelli, Modrzynska, Borges, Creasey, Rodrigues, Beraldi, Loewe, Fawcett, Kumar, Thomson, Trivedi, Otto, Pain, Blaxter and Cravo2010b), Henriques et al. (Reference Henriques, Martinelli, Rodrigues, Modrzynska, Fawcett, Houston, Borges, d'Alessandro, Tinto, Karema, Hunt and Cravo2013).

Atovaquone

Resistance to atovaquone (a chemical analogue of coenzyme Q) is readily achieved with the acquisition of mutations in the cytochrome bc1 complex both under laboratory conditions and in clinical field settings (Srivastava et al., Reference Srivastava, Rottenberg and Vaidya1997; Vaidya and Mather, Reference Vaidya and Mather2000). This was mirrored in RMPs as resistant to atovaquone has been selected for in P. berghei, P. yoelii and P. chabaudi (Srivastava et al., Reference Srivastava, Morrisey, Darrouzet, Daldal and Vaidya1999; Syafruddin et al., Reference Syafruddin, Siregar and Marzuki1999; Afonso et al., Reference Afonso, Neto, Castro, Lopes, Alves, Tomás and Rosário2010). The P. chabaudi atovaquone-resistant line was selected from the AS-3CQ (Fig. 4) line after stepwise dose escalation while resistant parasites in P. berghei and P. yoelii were selected from naïve parasite backgrounds. However, in all the three parasite species, genetic analysis revealed that the resistance phenotypes were due to mutations in the cytochrome bc1 complex even though independent reverse genetics have not been carried out to further validate their involvement. It should be noted that reverse genetics approaches could also be particularly difficult in these situations as the cytochrome bc1 complex is encoded by the mitochondrial genome.

Mefloquine

Until recently, the mechanism of action of and resistance to mefloquine has remained relatively elusive. An aryl aminoalcohol, mefloquine was initially believed to act by inhibiting haem polymerization within the parasite digestive vacuole while increased copy numbers of the multidrug resistance transporter (PfMDR1) have been implicated as a mechanism of resistance (Price et al., Reference Price, Uhlemann, Brockman, McGready, Ashley, Phaipun, Patel, Laing, Looareesuwan, White, Nosten and Krishna2004; Ecker et al., Reference Ecker, Lehane, Clain and Fidock2012). However, a more recent study has demonstrated that this drug can also act as a protein synthesis inhibitor in malaria parasites, specifically targeting the 80S ribosomal translational unit (Wong et al., Reference Wong, Bai, Sleebs, Triglia, Brown, Thompson, Jackson, Hanssen, Marapana, Fernandez, Ralph, Cowman, Scheres and Baum2017). Nevertheless, RMPs resistant to mefloquine have been selected and characterized. The most studied line is perhaps the AS-15MF which emerged from the AS drug selection panel of lines as described above (Fig. 4). This line was selected from a pre-existing chloroquine-resistant line (AS-15CQ) using an incremental dose of mefloquine until stable resistance at 15 mg kg⁻¹ was obtained. Linkage and genetic cross analysis of this line further revealed that increased expression of the PcMDR1 through copy duplication was indeed a constant feature of all resistant progenies which inherited the resistant phenotypes (Cravo et al., Reference Cravo, Carlton, Hunt, Bisoni, Padua and Walliker2003). However, further genetic analysis of the AS-15MF line also implicated the UBP-1 V2728F mutation (Hunt et al., Reference Hunt, Martinelli, Modrzynska, Borges, Creasey, Rodrigues, Beraldi, Loewe, Fawcett, Kumar, Thomson, Trivedi, Otto, Pain, Blaxter and Cravo2010b). Mefloquine resistant P. yoelii parasites have also been selected for, even though the genetic determinants have not been characterized (Merkli and Richle, Reference Merkli and Richle1983a). In P. berghei, cloning and sequencing of the PbMDR1 gene from a line which was selected for and attained stable resistance to mefloquine also revealed 2–3-fold amplification of this gene in resistant parasites as compared to the sensitive wild type (Gervais et al., Reference Gervais, Trujillo, Robinson, Peters and Serrano1999). In these circumstances, even though the 80S ribosome might be the direct target of mefloquine, it can be relatively difficult to fully pinpoint the mode of action as UBP-1 and MDR1 which are implicated in the mode of resistance (just like with gene amplifications observed with antifolates, discussed above) could be involved with transport or efflux of the drug.

Chloroquine

Since resistance to chloroquine emerged in P. falciparum in the 1970s, the mode of resistance remained poorly characterized until the early 2000s (Ecker et al., Reference Ecker, Lehane, Clain and Fidock2012). This is because it proved specifically difficult to select for chloroquine resistance in P. falciparum under laboratory culture conditions from naïve parasite strains. Identification of the chloroquine resistance transporter (PfCRT) as the principal determinant of resistance involved detailed genomic, biochemical and allele exchange experiments to identify a 13-exon gene within a 36 kb chromosomal fragment that strongly associated with chloroquine resistance phenotypes in resistant parasites (Fidock et al., Reference Fidock, Nomura, Talley, Cooper, Dzekunov, Ferdig, Ursos, Sidhu, Naudé, Deitsch, Su, Wootton, Roepe and Wellems2000). RMPs have, however, provided an additional route to understanding chloroquine resistance as even though it has proved to be difficult to generate parasites with stable resistant phenotypes, a number of lines have been reported. The most widely studied RMP models of chloroquine resistance are from the P. chabaudi AS lineage as described in sections above (Fig. 4). The AS-3CQ was the first P. chabaudi line with a stable chloroquine resistance phenotype (Rosario, Reference Rosario1976). In this line, initial biochemical analysis revealed reduced accumulation of chloroquine in the resistant parasites as compared to their sensitive counterparts (Ohsawa et al., Reference Ohsawa, Tanabe, Kimata and Miki1991). Subsequent quantitative genome sequence analysis of the AS-3CQ line also identified a single mutation in an amino acid transporter aat (PCHAS_1127800) that could be a possible determinant of this drug resistance phenotype (Kinga Modrzynska et al., Reference Kinga Modrzynska, Creasey, Loewe, Cezard, Trindade Borges, Martinelli, Rodrigues, Cravo, Blaxter, Carter and Hunt2012). However, reverse genetics approaches have not been carried out to further validate its contribution. Meanwhile, further selection of the AS-3CQ line generated higher degree chloroquine resistance lines (AS-15CQ and AS-30CQ), both of which carried UBP-1 mutations (V2697F and V2728F) as genetic determinants (Hunt et al., Reference Hunt, Afonso, Creasey, Culleton, Sidhu, Logan, Valderramos, McNae, Cheesman, do Rosario, Carter, Fidock and Cravo2007, Reference Hunt, Martinelli, Modrzynska, Borges, Creasey, Rodrigues, Beraldi, Loewe, Fawcett, Kumar, Thomson, Trivedi, Otto, Pain, Blaxter and Cravo2010b). P. berghei strains resistant to chloroquine have also been selected and reported which, however, has in most cases resulted in relatively unstable phenotypes. In some of the early works, exposure of P. berghei parasites to chloroquine supplied in animal diet for 4 months resulted in highly resistant strains that easily tolerated above maximum effective doses of the drug under standard treatment conditions (Hawking, Reference Hawking1966). These chloroquine-resistant parasites also displayed a cross-resistance phenotype to other drugs such as sulphadiazine and pyrimethamine. However, the phenotype was easily lost and could not be resuscitated when drug pressure was reapplied. Around the same time, other unstable chloroquine-resistant P. berghei RC strains that displayed up to 60-fold resistance as compared to the wild type were also reported (Peters, Reference Peters1965). The only P. berghei parasites with stable chloroquine-resistant phenotypes were reported in 1998. These lines were selected from the NK65 line with an incremental dose of chloroquine ranging from 1, 3, 6, 10 through to 30 mg kg⁻¹. From each of these doses, stable phenotypes were obtained at various levels of the drug selection (CQR3, CQR6, CQR10 and CQR30) which, crucially, displayed high-level resistance in both the P. berghei in vitro short-term assay as well as in vivo (Platel et al., Reference Platel, Mangou and Tribouley-Duret1998). Nevertheless, the genetic determinants of the chloroquine resistance phenotypes in these lines have not been characterized.

Allelic exchange and Crispr-Cas9: of malaria mutant models in mice, a new approach?

RMPs (except P. vinckei) are easily amenable to genetic manipulation as they demonstrate higher transfection efficiency as compared to P. falciparum (Janse et al., Reference Janse, Franke-Fayard, Mair, Ramesar, Thiel, Engelmann, Matuschewski, Gemert, Sauerwein and Waters2006; Jongco et al., Reference Jongco, Ting, Thathy, Mota and Kim2006). Reverse genetics approaches by introducing P. falciparum drug resistance alleles in rodent parasites through allelic exchanges have been pursued in order to assess drug resistance phenotypes in vivo (Fidock et al., Reference Fidock, Rosenthal, Croft, Brun and Nwaka2004). PfCRT mutant forms responsible for chloroquine resistance have been introduced in P. berghei (Ecker et al., Reference Ecker, Lakshmanan, Sinnis, Coppens and Fidock2011). Even though these PfCRT alleles did not result in equivalent chloroquine resistance phenotypes as observed in P. falciparum, it was demonstrated that under drug pressure, P. berghei parasites carrying PfCRT mutant forms achieved better and efficient transmission. An inherent disadvantage of such approaches is that it involves the introduction of a transgene into parasites that maintain normal expression of the internal loci irrespective of how conserved the alleles are between the spp. In such situations, it is difficult to quantify drug resistance phenotypes especially if the markers under study occur in proteins or enzymes that do not respond to (trans)gene dosage or if the background expression is sufficient to overshadow any resulting phenotype from the introduced alleles. However, with the development of recent highly precise genome editing technologies such as CRISPR-Cas9, instead of introducing P. falciparum antimalarial drug-resistant candidate alleles in RMPs as transgenes, orthologous polymorphisms can be introduced with precision in attempts to characterize phenotypes based on assumed gene function conservation. Such CRISPR approaches have recently been used in P. berghei in vivo to validate UBP-1 and Kelch13 ART resistance mutations which were first identified in P. chabaudi and P. falciparum, respectively (Simwela et al., Reference Simwela, Hughes, Roberts, Rennie, Barrett and Waters2020a, Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b). Even though evolutionary divergence between RMPs and P. falciparum means overall protein sequence identities cannot be always highly conserved (e.g. P. berghei and P. falciparum UBP-1 share 41% sequence identity), there appears to be a reasonable degree of similarity in the functional domains (Simwela et al., Reference Simwela, Hughes, Roberts, Rennie, Barrett and Waters2020a). Meanwhile, certain drug resistance genes are highly conserved, for instance P. berghei and P. falciparum Kelch13 share over 80% sequence identity (Simwela et al., Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b). In either cases, these features have been exploited in CRISPR-Cas9 mediated reverse genetics approaches to confirm the causality of drug resistance mutant alleles in in vivo conditions (Simwela et al., Reference Simwela, Hughes, Roberts, Rennie, Barrett and Waters2020a, Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b) which has at times been problematic or debatable using in vitro systems in P. falciparum (Sá et al., Reference Sá, Kaslow, Krause, Melendez-Muniz, Salzman, Kite, Zhang, Moraes Barros, Mu, Han, Mershon, Figan, Caleon, Rahman, Gibson, Amaratunga, Nishiguchi, Breglio, Engels, Velmurugan, Ricklefs, Straimer, Gnädig, Deng, Liu, Diouf, Miura, Tullo, Eastman, Chakravarty, James, Udenze, Li, Sturdevant, Gwadz, Porcella, Long, Fidock, Thomas, Fay, Sim, Hoffman, Adams, Fairhurst, Su and Wellems2018). The introduced Kelch13 and UBP-1 mutations in P. berghei (F448I, Y505H, M488I, R551T for the former and V2721F, V2728F for the latter) all resulted in ART or chloroquine resistance phenotypes just like their P. falciparum and P. chabaudi equivalents which were reversible when some of these mutations were reversed or repaired (Simwela et al., Reference Simwela, Hughes, Roberts, Rennie, Barrett and Waters2020a, Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b). Moreover, mutant P. berghei parasites carrying drug resistance alleles (UBP-1 and some Kelch13) possessed fitness defects which are easily assessed and quantified in RMPs under physiologically relevant in vivo conditions. In SEA, Kelch13 mediated ART resistance is primarily associated with the C580Y mutation (Hamilton et al., Reference Hamilton, Amato, van der Pluijm, Jacob, Quang, Thuy-Nhien, Hien, Hongvanthong, Chindavongsa, Mayxay, Huy, Leang, Huch, Dysoley, Amaratunga, Suon, Fairhurst, Tripura, Peto, Sovann, Jittamala, Hanboonkunupakarn, Pukrittayakamee, Chau, Imwong, Dhorda, Vongpromek, Chan, Maude, Pearson, Nguyen, Rockett, Drury, Gonçalves, White, Day, Kwiatkowski, Dondorp and Miotto2019; van der Pluijm et al., Reference van der Pluijm, Imwong, Chau, Hoa, Thuy-Nhien, Thanh, Jittamala, Hanboonkunupakarn, Chutasmit, Saelow, Runjarern, Kaewmok, Tripura, Peto, Yok, Suon, Sreng, Mao, Oun, Yen, Amaratunga, Lek, Huy, Dhorda, Chotivanich, Ashley, Mukaka, Waithira, Cheah, Maude, Amato, Pearson, Gonçalves, Jacob, Hamilton, Fairhurst, Tarning, Winterberg, Kwiatkowski, Pukrittayakamee, Hien, Day, Miotto, White and Dondorp2019). Intriguingly, P. berghei equivalent of the C580Y (C592Y) mutation and the other important Kelch13 mutation, R539T (R543T) could not be introduced in this RMP in several attempts despite a high degree of conservation of the predicted Kelch13 structures and mutation locale between the two parasites (Simwela et al., Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b). The level of Kelch3-mediated ART resistance (notably with the C580Y substitution) and the resulting fitness thereof is also dependent on the parasite genetic backgrounds (Straimer et al., Reference Straimer, Gnädig, Witkowski, Amaratunga, Duru, Ramadani, Dacheux, Khim, Zhang, Lam, Gregory, Urnov, Mercereau-Puijalon, Benoit-Vical, Fairhurst, Ménard and Fidock2015) which donate compensatory architectures to cushion the deleterious effects of the mutations (Miotto et al., Reference Miotto, Amato, Ashley, MacInnis, Almagro-Garcia, Amaratunga, Lim, Mead, Oyola, Dhorda, Imwong, Woodrow, Manske, Stalker, Drury, Campino, Amenga-Etego, Thanh, Tran, Ringwald, Bethell, Nosten, Phyo, Pukrittayakamee, Chotivanich, Chuor, Nguon, Suon, Sreng, Newton, Mayxay, Khanthavong, Hongvanthong, Htut, Han, Kyaw, Faiz, Fanello, Onyamboko, Mokuolu, Jacob, Takala-Harrison, Plowe, Day, Dondorp, Spencer, McVean, Fairhurst, White and Kwiatkowski2015). In these cases, CRISPR-Cas9 genome editing in RMP as applied in P. berghei can provide useful information on the evolution of drug resistance in malaria parasites by revealing the impacts of specific mutations on naive parasite backgrounds. Experimental tractability of RMPs could also mean such mutant parasites could be assessed for transmission fitness in the absence and or presence of drug pressure. These mutant RMPs are also offering opportunities to assess the ex vivo and in vivo efficacy of antimalarial agents which can be used as combinational partners with ARTs to offset resistance (Simwela et al., Reference Simwela, Stokes, Aghabi, Bogyo, Fidock and Waters2020b, Reference Simwela, Hughes, Rennie, Barrett and Waters2021).