Open access peer-reviewed chapter - ONLINE FIRST

Progress in Parasite Genomics and Its Application to Current Challenges in Malaria Control

By Cheikh Cambel Dieng, Colby T. Ford, Jennifer Huynh, Linda E. Amoah, Yaw A. Afrane, Daniel A. Janies and Eugenia Lo

Submitted: October 5th 2020Reviewed: February 9th 2021Published: March 19th 2021

DOI: 10.5772/intechopen.96530

Downloaded: 34

Abstract

A wide deployment of malaria control tools have significantly reduced malaria morbidity and mortality across Africa. However, in the last five to seven years, there has been a resurgence of malaria in several African countries, raising the questions of whether and why current control mechanisms are failing. Since the first Plasmodium falciparum reference genome was published in 2002, few thousands more representing a broad range of geographical isolates have been sequenced. These advances in parasite genomics have improved our understanding of mutational changes, molecular structure, and genetic mechanisms associated with diagnostic testing, antimalarial resistance, and preventive measures such as vaccine development. In this chapter, we summarize the current progress on: (1) genomic characteristics of P. falciparum; (2) novel biomarkers and revolutionary techniques for diagnosing malaria infections; and (3) current vaccine targets and challenges for developing efficacious and long-lasting malaria vaccines.

Keywords

  • genomics
  • Plasmodium falciparum
  • malaria diagnosis
  • bioinformatics
  • antimalarial resistance
  • malaria vaccines
  • biomarkers
  • genetic diversity

1. Introduction

Malaria remains a serious public health problem in several developing countries. Globally, there are about 3.2 billion people at risk of malaria and 435,000 malaria-related deaths, most of which happening in West Africa [1, 2]. Malaria is a complicated disease caused by the genus Plasmodiumin the protozoan phylum Apicomplexa. While P. falciparumis the most prevalent form of malaria, P. vivaxis most widespread around the world. Plasmodiumhas a complicated life cycle that reproduces asexually in human and sexually in mosquito hosts. The parasite is transmitted by the female Anophelesmosquitoes. Anophelesmosquitoes thrive in warm, tropical climates as the temperature allows for quicker breeding and hatching [3]. The abundance of vectors is positively correlated with the transmission rate of malaria [4]. People infected with malaria normally experience fever, chills, diarrhea, vomiting, and anemia [5]. If remain untreated, the disease can progress to a severe form and result in death [6].

A wide deployment of malaria control tools in the past few decades have significantly reduced malaria morbidity and mortality worldwide. The number of countries with fewer than 100 clinical malaria cases increased from six to 27. Countries including Iran, Malaysia, Timor-Leste Belize, Cabo Verde, China, and El Salvador reported zero malaria cases in 2019 and malaria cases dropped by 90% in the Greater Mekong subregion (GMS) [7]. However, in the last five to seven years, there has been a resurgence of malaria in several African countries, raising the questions of whether and why current control mechanisms are failing. A number of factors has limited malaria control and elimination efforts. First, Plasmodiumisolates may respond differently to antimalarial drugs, with some evolved to become more resistant than the others due to prolonged drug use. Second, multiplicity of infection (MOI), i.e., the number of Plasmodiumisolates co-infecting a single host, has made molecular characterization of the parasites and understanding of disease severity difficult [8]. Third, diagnostic inaccuracy related to false negative results by rapid diagnostic tests (RDTs) is becoming a more widespread phenomenon [9]. Other factors such as asymptomatic reservoirs leading to transmission, lack of effective vaccine, and warmer climates and changing environments caused by human activities [10] have also hampered malaria elimination efforts. Thus, it is critically important to create new tools that allow us to monitor parasite changes and use that information to improve existing control strategies. In this chapter, we will summarize the current progress on: (1) genomic characteristics of P. falciparum; (2) novel biomarkers and revolutionary techniques for diagnosing malaria infections; and (3) current vaccine targets and challenges for developing efficacious and long-lasting malaria vaccines.

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2. Genomic characteristics of Plasmodium falciparum

Knowledge of the evolution and genetic variation of the Plasmodiumgenome offers incredible insights into novel means of malaria diagnosis and treatment. The advances in parasite genomics have improved our understanding of mutational changes, molecular structure, and genetic mechanisms associated with failure in diagnostic testing [11], antimalarial resistance [12], and preventive measures such as vaccine development [13]. Since the first reference genome of P. falciparumwas published in 2002 [14], several thousand DNA sequences have been collected and deposited in public databases. Plasmodium falciparumgenome is approximately 23.7 Mb with 14 chromosomes, a plasmid of about 35 kb, and lots of mitochondrial DNA copies of about 6 kb [15]. There are currently 5,438 genes that have been predicted/discovered within the genome with 33% uncertainty of their functions [16]. The genome contains many rich AT regions in both exons and introns (80% and 90%, respectively), which has some advantages and disadvantages when learning more about the genetic architecture of the parasites [17]. The advantage associated with the genomic data would be using its rich polymorphic AT content as biomarkers to map out the evolutionary structure of the parasites and correlating it with any drug resistant genes [15]. Although having a rich AT genome has contributed to a high yield in microsatellites or simple sequence repeats, there are some disadvantages when using the genome in genetic studies [15]. For example, within CRISPR-Cas9, the high AT content resulted in a decrease in the amount of gRNA target sites needed [18]. A deeper knowledge of the genome’s polymorphic and conserved genes are therefore essential towards understanding the evolutionary timeline of various P. falciparumlineages.

Compared to other eukaryotic organisms, whole genome sequencing (WGS) showed that the genome of P. falciparumcontains fewer genes for enzymes and transporters, but more genes for immune evasion to support host–parasite interactions [14]. With an average length of 2.4 Kb, P. falciparumgenes are considerably larger than many organisms. P. falciparum’s genome contains a full set of transfer RNA (tRNA) ligase genes with minimal redundancy. 43 tRNAs have been identified to bind all codons except TGT and TGC, which code for cysteine, thus giving P. falciparuma slightly different amino acid translation than is seen in humans and other eukaryotes. By contrast, the mitochondrial genome of P. falciparumis only about 6Kb and does not contain any genes that encode for tRNAs, implying that the mitochondrion must import tRNAs from elsewhere into the cells [19, 20]. Polymorphic genes in the P. falciparumgenome are useful in creating linkage maps to monitor mutational changes and genetic diversity of the parasites in response to malaria interventions and control efforts [21]. Polymorphic genes are variations in genes at higher frequencies that can be advantageous, neutral, or disadvantageous [22]. The role of polymorphic genes is to influence coding regions, alter protein sequences and gene expression, and eventually the metabolic pathway and function [23]. For example, remarkable polymorphisms observed in the merozoite surface proteins (MSP), PfAMA1, PfEBA, and PfRHsgenes that involved in merozoite evasion have been shown to increase the evasion ability of P. falciparumto the host immune system [24].

In comparison, conserved genes are genes that have not been altered. They contribute to important biological processes and fitness [25]. Information of conserved genes allow us to infer phylogenetic relatedness and trace the genetic origin of different lineages, determine new targets for therapeutic treatment, and serve as a guide when determining functions of unknown genes [18]. The processes that determine the polymorphisms of the parasitic genome include both selective pressures and recombination frequencies. Selective pressures on conserved genes allow certain important genes to remain unmodified for normal metabolic activities, whereas polymorphic genes diversify through frequent recombination allow for better evasion of antimalarial drug treatments and escape detection from diagnostic tests [26]. For example, the PfHRP2gene has shown with partial deletions and/or mutations over the past few years due to the usage of HRP2-specific Rapid Diagnostic tests (RDTs) [27, 28]. More specifically, the histidine-rich repeats in the PfHRP2gene drastically change the length of the gene and the ability of the parasites to evade RDTs. Therefore, novel genes that encode for parasite specific function might be potential new targets for malaria diagnosis and/or treatment [14]. It is important to distinguish metabolic pathways that the parasites use for invasion of the host cells as well as evasion of the host immune system.

P. falciparumis clearly genetically distinct by geographical regions [29, 30]. Given the complex life cycle of Plasmodium, genomic data coupled with Genome-Wide Association Studies can offer deep insights into the tangled relationships among humans, mosquitoes, and the parasites. To date, databases such as PlasmoDB have integrated sequence information, functional genomics, and annotation of data emerging from the P. falciparumgenome sequencing consortium [31]. These databases provide an important platform to retrieve biological meaning from new ‘omic’ data and enhance diagnosis and treatment of infections caused by this dreadful malaria pathogen.

3. Conventional and novel methods for malaria diagnosis

One of the challenges to malaria elimination is the burden of submicroscopic asymptomatic infections that contribute to malaria transmission [7]. The gold standard for malaria diagnosis is microscopy [32]. Microscopy can differentiate malaria species and quantify parasite density, but only has a detection threshold of 10 to 50 parasites μl of blood (approximately 0.001% parasitemia, assuming an erythrocyte count of 5 × 106 cells μl) [33]. However, it requires well trained microscopists and is labor-intensive and time-consuming [32]. Previous studies have reported higher prevalence of asymptomatic parasitemia (6–7 times higher) using PCR compared to microscopy [5]. Nested PCR of the 18 srRNA genes has been commonly used to detect submicroscopic infections. PCR-based methods are also more sensitive than microscopy at detecting gametocytes particularly in asymptomatic individuals with low-density infections [34]. However, recent studies indicated a relatively high number of misdiagnosed infections [9], possibly due to low parasite density being less detectable by conventional PCR. The 18 srRNA gene has a reported detection thresholds of 0.5–5 parasites μl [35], but parasite density of asymptomatic infections especially in low transmission settings could be well below this threshold. As a result, many of these infections remain undetected in the general populations of several malaria-endemic countries [10, 36, 37] and provide perfect reservoirs for transmission at any time. Therefore, it is crucial to identify new gene targets or novel tools that are convenient and affordable for detecting asymptomatic infections, particularly in countries approaching elimination phase. Below are comparisons of various conventional and novel detection methods.

3.1 Rapid diagnostic test (RDT)

Rapid Diagnostic Test (RDT) is a lateral flow immunochromatographic test that can detect the presence of Plasmodiumparasites by using blood from patients. The blood samples collected from patients must be lysed before the Plasmodiumantigens being stained. RDT will indicate if the patient has malaria or not [38]. This diagnostic method is useful in rural areas as it is inexpensive and does not require expertise to perform the test [38]. There are various types of RDTs that can detect different antigens of Plasmodiumparasites including P. falciparumand P. vivax, namely P. falciparumhistidine-rich protein 2 (PfHRP2) and lactate dehydrogenase (PfLDH). However, recent studies indicated that parasites lacking the pfhrp2/pfhrp3genes could result in false-negative PfHRP2-RDT results, and these pfhrp2/pfhrp3variants have been spreading in many East and West African countries [39, 40, 41, 42]. Reports of deletion of HRP2and HRP3genes was first reported in 2010 within the Peruvian Amazon [43] and the number of false negative RDTs has substantially increased in late 2014 [44]. Prevalence of false negative cases related to HRP2deletions in South America (with the exception of Peru) is lower than Asia and Sub-Saharan Africa [45]. The highest prevalence (50% pfhrp2deletions among all positive cases) were reported in Cambodia, Peru, and Eritrea [46]. Such a high prevalence could be explained by technical errors, mutations, selection and spread of the pfhrp2and 3 variants [47] from South America to Africa and Asia [41]. Recently, a novel HRP2-based Alere™ Malaria Ag P.f RDT (uRDT) was developed specifically for the detection of asymptomatic infections. Compared to the existing RDTs, the uRDT showed a greater than 10-fold improvement in diagnosing clinical and asymptomatic cases [48]. However, the sensitivities of the uRDT were inconsistent among different transmission settings [49]. Thus, although very promising for the detection of asymptomatic infections, the performance of uRDT must be further evaluated especially in areas with a already high prevalence of pfhrp2and pfhrp3gene deletions.

3.2 Enzyme-linked immunosorbent assay (ELISA)

ELISA is an enzyme-linked immunosorbent assay that is used to detect antigens and antibodies by utilizing a highly specific antibody–antigen interaction and their bonding affinity to proteins on a solid surface [50]. Samples, including and positive and negative controls are inserted on a 96 well plate which enables the possibility to analyze multiple samples simultaneously, then samples get incubated and detection of the signal is generated directly or indirectly via secondary tag on the specific antibody [51]. ELISA can be very efficient diagnostic tool for Plasmodiumbecause it is highly specific and sensitive and therefore can be used to screen blood donors and pregnant women who may or may not have been exposed to the parasite [1]. However there are some limitations associated with using ELISA, as it is unable to detect antibodies in patients with acute infections, patients with different Plasmodiumspecies, and various antigens within the different life stages of the parasite [52]. A recent study showed a lower detection threshold (3 parasites/μl) by ELISA test of the Plasmodiumlactate dehydrogenase (pLDH) as compared to RDT (50–60 parasites/μl) [53]. However, ELISA has a lower sensitivity (69.9%) to antigens than RDT (88%) [53], and can be expensive and require a trained technician to operate and interpret the results [53].

3.3 Lateral flow immunoassay (LFIA)

One of the current diagnostic tests in development is an antibody-based lateral flow immunoassay (LFIA). Unlike ELISA that requires repeated incubation and washing steps, LFIA is considered to be a simple, user-friendly and cost-effective method for front-line diagnosis [54]. LFIA is versatile enough to detect target genes in sample matrices including whole blood, saliva, and urine. This method is primarily applied to detecting gametocytes in malaria-infected samples. Gametocytes are the sexual form of the parasite that gets transmitted to the mosquito host. They play a very important role in malaria transmission, and can contribute to up to 80% [55] of the infectious reservoirs. Previous studies have shown that infections with parasitemia as low as 4 gametocytes/μl can sustain transmission [56]. LFIA targets Pfs25in infected blood samples, which is a glycophosphatidylinositol-linked protein expressed on the surface of P. falciparumzygotes and ookinetes but only found on female gametocytes in the human hosts [57]. The detection limit of Pfs25LFIA is 0.02 gametocytes/μl, much more sensitive than pfhrp2RDT with a detection limit of 50–100 parasites per μL of blood [35, 58]. Another protein at the surface of the female gametocyte PSSP17, which is presumably more abundant in saliva samples, was also investigated in Cameroon, Zambia and Sierra Leone with an estimated sensitivity of 83% (95% CI, 61 to 95) in symptomatic patients when compared to PCR as the gold standard [58]. Detection of pfhrp2in saliva have been reported recently using LFIA, but the sensitivity was only shown to be improved in severe to moderate form of infections with parasitemia >60,000 parasites/μL [59]. Although convenient, pfhrp2-based LFIA could be less useful in detecting asymptomatic infections.

3.4 PCR-based methods

The combination of PCR-based assays and sequencing technologies have revolutionized malaria diagnosis since their introduction in the early 2000s. Various gene targets have be used to monitor genetic and/or mutational changes in the parasites that cause the disease. PCR is a very common technique used in malaria diagnoses in laboratory settings. The main advantage of this technique is that it enables us to identify individuals with low parasitemia (Table 1). There are multiple versions of this technique including nested conventional PCR, real-time quantitative PCR and reverse transcriptase PCR. Nested PCR is the easiest and least expensive methods among the others. It only requires a thermocycler, set of primers, reagents and visualization after gel electrophoresis. It is mostly a qualitative method as it is fairly difficult to estimate parasite density on a agarose gel. Unlike conventional PCR that uses gel electrophoresis to visualize PCR products, real-time PCR or qPCR detects and quantifies the amount of amplified DNA usually by SYBR green or a fluorogenic probe designed based on a target gene segment (TaqMan). The standard cycle threshold (Ct) value is inversely proportional to the amount of target DNA in the sample [66] and allows estimation of parasite density even in submicroscopic samples. Different from nested and qPCRs, reverse transcriptase PCR uses RNA as template and transcribes RNA into complementary DNA. This method has been widely used to detect and quantify gametocyte density in malaria samples. Though PCR-based methods are undoubtedly more sensitive than microscopic diagnosis, the level of sensitivity is highly dependent on the gene targets (Table 1).

TypeTargetSensitivity (%)Specificity (%)ApplicationDetection LimitRefs
RDTHRP2/35799Field50–100 parasites/μL of blood[35]
RDTLDH5893Field50–100 parasites/μL of blood[35]
PCR18 srRNA6492Laboratory0.5–5 parasites/μL of blood[60]
PCRCOX3Laboratory0.6–2 parasites/μL blood[60]
PCRTARE-28149Laboratory6–24 parasites in 200 μL whole blood[61]
PCRvarATSLaboratory12–30 parasites in 200 μL whole blood[62]
PCRPfs25Laboratory0.3 mature females/μL blood[63]
ELISALDH69.9100Laboratory3 parasites/μL blood[53, 64]
LFIAPfs25Laboratory0.02 gametocytes/μl blood[58]
SERSHemozoinLaboratory30 parasites/μL of blood[65]

Table 1.

Existing malaria diagnostic tests and their respective performance.

— Denotes that the sensitivity or specificity is not reported.

3.4.1 18 s rRNA

The 18 srRNA genes have been the main gene target for molecular screening as it contains 5–8 copies per genome [62] in Plasmodium, but recent studies indicated a relatively high level of misdiagnosed infections [45]. The advantage of using the 18 srRNA is that it is highly specific compared to microscopy or RDT diagnoses. The primer sequences and protocols for both nested and qPCRs have been readily established. However, it fails to reveal infections with low parasite density (0.5–5 parasites/μL of blood) [35]. Thus, new target genes have been examined in the past few years with the goal to achieve an ultra-sensitive biomarker with higher sensitivity and specificity compared to the 18 srRNA.

3.4.2 Mitochondrial cytochrome c oxidase III (COX3)

The cytochrome c oxidase III (COX3) gene plays a very important role in cellular respiration [67]. It is a mitochondrial gene that inherited solely from the female gametocyte and less likely to undergo genetic recombination, making it an ideal candidate for identifying the origin and transmission of the parasites [68]. More importantly, there are around 20 to 150 copies of the COX3gene in the Plasmodiumgenome [62] and PCR analysis of this gene indicated a detection limit of 0.6–2 parasites/μL, much more sensitive than the 18 s-rRNA [60].

3.4.3 Telomere associated repetitive element 2 (TARE-2)

The recently discovered Telomere Associated Repetitive Element 2 (TARE-2) has demonstrated better performance than the conventional 18 srRNA marker in detecting low density parasite infections. There are about 250 copies of the TARE-2gene in the Plasmodiumgenome and this gene is highly specific to P. falciparum[69]. TARE-2has been previously shown to be useful for detecting ultra-low density P. falciparuminfections in Papua New Guinea and Tanzania [62]. A recent study in Ghana showed a slightly higher sensitivity of TARE-2compared to 18 srRNA (81.2% vs. 80.9%) using microscopy as a gold standard, but with a lower specificity reduced by almost two-fold [37], making this gene less desirable for active case surveillance.

3.4.4 Var. gene acidic terminal sequence (varATS)

The vargene family is located primarily in the subtelomeric region of the Plasmodiumgenome. It is a family of genes known to be highly polymorphic. For instance, the genome of the 3D7 culture strain harbors 59 different vargenes with an estimated 50–150 copies per genome [14]. One of the main gene in the vargene family encodes the P. falciparumerythrocyte membrane protein 1 (PfEMP1) that contains a highly variable extracellular part and a well conserved intracellular vargene acidic terminal sequence (varATS) [61]. The varATS has a detection limit of 12–30 parasites in 200 μL whole blood. Though more sensitive 18 srRNA, varATS employs a qPCR approach that could be less feasible for routine case detection in rural areas or developing countries [62].

3.5 Raman spectroscopy

Raman spectroscopy is a relatively novel technique that can be used to diagnose the presence of Plasmodium. This technique measures the amount of wavelength and light intensity of scattered light reflected from the target molecule of Plasmodiumpresent in an infected sample either in liquid, gas, or solid form [70]. Raman spectroscopy can be used specifically to characterize hemozoin, a pigment produced by infected erythrocytes and can be used to track the progression of the disease and efficacy of drug treatment [71]. A specific type of Raman spectroscopy known as Surface Enhanced Raman Spectroscopy (SERS) has been utilized to detect early signs of erythrocytic infections and was shown with a detection limit of 30 parasites/μL [65]. Tip-enhanced Raman spectroscopy (TERS), on the other hand, can enhance Plasmodium’s hemozoin vacuole from 106 to 107 [71]. While Raman spectroscopy is more cost effectiveness than PCR and microscopy [71], this technique cannot detect hemozoin in early ring stage nor differentiate hemozoin from active and previous infections [71]. Further investigations are needed to refine Raman signals in order to enhance the technique’s detection abilities.

4. Revolutionized techniques and genomics tools for monitoring parasite changes

Extensive level of genetic diversity observed in Plasmodiumis a major threat to the eradication of the disease. Previous studies used sanger sequencing of the merozoite surface protein (MSP) or microsatellite genotyping methods to assess parasite genetic diversity. Though affordable, these methods are time-consuming and labor-intensive for large scale genetic studies. Moreover, differentiating or phasing clonal genotypes for samples with more than two clones can be difficult. Restriction enzyme cutting followed by gel electorphoresis of the MSP gene has been conventionally used to assess parasite diversity and define multiplicity of infections (MOI) based on the number of distinct bands present on a gel. MSP is the most abundant protein at the surface of the merozoite and play a critical role in the Plasmodiuminvasion mechanism to the erythrocyte [72]. It is an informative gene for resolving clonal relationships and depicting population structure of Plasmodiumgiven its size polymorphisms [73]. However, in high transmission areas where parasites are highly variable and different by single nucleotide polymorphisms (SNPs), gel electorphoresis of the MSP gene would underestimate the levels of diversity and polyclonality [74]. Microsatellite genotyping has also extensively been used for Plasmodiumpopulation structure and genetic diversity study [75]. While this marker has the advantages of being polymorphic, evolutionary neutrally, and are abundant in the Plasmodiumgenome [76], polyclonal samples with more than two alleles detected from two or more genetic loci are usually discarded in the analyses. Thus, next-generation sequencing (NGS) technologies offer a novel, alternative approach to shed light on the polyclonal and complex nature of Plasmodiuminfections [77].

4.1 Amplicon deep sequencing

In regions in high malaria endemicity, individuals typically harbor multiple Plasmodium falciparumisolates due to repeated exposure to mosquitoes infected with multiple parasite isolates [78]. Polyclonal infections have become a growing concern as some parasite isolates may be resistant to antimalarial drugs and/or more pathogenic [79]. Identification of genetically distinct clones is necessary to critically evaluate the causation of resistance to drugs and any other therapeutic treatments. Recently, due to reduced cost of high throughput NGS technology, other types of molecular tools have emerged to address the complex issue related to MOI. MOI is defined as the number of parasite clones within an infected sample. Deep sequencing of a targeted gene amplicon coupled with bioinformatic analyses allow differentiation of various P. falciparumstrains based on SNPs [75] and discrimination of major from minor clones [80]. It also provides an increased capability to detect the genetic relatedness among clones within and between hosts as well as minor P. falciparumvariants [81]. This technique can be applied to different gene regions such as Circumsporozoite (CSP), MSP1/2, and Apical membrane antigen (AMA) to monitor changes as well as selection pressure acting on the parasite populations [82].

4.2 Molecular inversion probe

Molecular inversion probes (MIPs) are another deep sequencing technique that targets several short gene regions across the genome. MIPs are single stranded DNA molecules that contain flanking regions of the targeted gene regions up to several hundred base pairs long [83]. MIPs can hybridize with the target sequence and undergo gap filling ligation to form circular DNA. The target sequence will also contain adaptors and barcodes to be further amplified by PCR [83]. The advantages of this technique include low rate of errors, small amount of DNA samples, high throughput, and cost-effective for several hundreds of samples. It is scalable to the number of targeted gene regions and samples, requires minimal costs in terms of reagents and labor, and allows efficient capture of DNA extracted from dried blood spots [84]. The latter advantage would make large-scale population studies feasible. MIPs have been used for monitoring SNP mutations associated with drug resistance, such as crt, mdr1, dhps, dhfr, and K13(Table 2) [84]. For example, a recent study based on MIPs analysis found that the PfDHPSgene associated with Sulfadoxine resistance has been rapidly spread from east to west of the Democratic Republic of Congo [84]. Apart from drug-resistant mutations, a number of microsatellite loci have also been added to the MIP panel to estimate genetic structure and diversity of P. falciparum. This technique allows multiple loci to be genotyped simultaneously. However, the design of the MIP panel would require prior information of the gene regions of interest.

Anti-malarialChloroquineAmodiaquineSulfadoxinePyrimethamineArtemisinin
GeneCrtMdr1DhpsDhfrK13
Mutation(s)K76TN86Y, Y184FA437G, K540EN51I, C59R, S108NM476I, Y493H, R539T, I543T, C580Y

Table 2.

Gene mutations associated with antimalarial drug resistance.

5. From parasite genes to malaria vaccines

Genetic information of P. falciparumhas allowed a careful selection of gene targets for vaccine development [85]. Vaccines can offer protection against clinical malaria especially in young children and reduce transmission in a population. However, there are several challenges in developing a highly effective malaria vaccine, mostly due to the complexity in the parasite life cycle and host immune system. Plasmodiumparasites reproduce asexually in human hosts. They can be found throughout the body’s bloodstream and liver in various stages. There are numerous potential parasite antigens that elicit different levels of host immune response [86], but the protective response towards a particular antigen or one parasite life-stage is not effective in conferring protection against other stages [87]. One solution for that is to choose an immunogenic antigen/epitope that can elicit a strong immune response and potentially confer the highest efficacy. Conjugating the target antigen or epitope with an adjuvant or better drug delivery system can help elicit a stronger and safer immune response [88]. Alternatively, it is also possible to activate other immune cells such as natural killer cells and neutrophils that can elicit a long-lasting immune response [89]. Natural killer cells act faster than T cells while neutrophils can activate either a humoral or cell mediated immunity [90]. Both natural killer cells and neutrophils in response to P. falciparuminvasion have not been studied in depth compared to antibodies and T cells [90]. To date, there are three types of malarial vaccines that are being studied and tested in clinical trials: pre-erythrocytic, erythrocytic, and transmission blocking vaccines (Table 3).

Name of VaccineType of VaccineTarget of VaccineMalarial Life Cycle StagePhase of VaccineEfficacyRefs
RTS,S/AS01ERecombinant protein vaccineCircumsporozoite protein (CSP)Pre-ErythrocyticPhase III35.2% in Children 20.3% in Infants[94]
PfSPZLive, radiation- attenuated vaccineSporozoite (SPZ)Pre-ErythrocyticPhase IIIHomologous challenge: 64% Heterologous challenge: 83%[102]
PfLSAVaccineRecombinant protein vaccineLiver-stage antigen 1 (LSA-1)Pre-ErythrocyticPhase IEfficacy has yet to be found in humans[105]
MSP1VaccineSubunit based VaccineMSP1ErythrocyticPhase IEfficacy has yet to be found in humans[110]
AMA-1VaccineRecombinant protein vaccine?AMA-1ErythrocyticPhase IIEfficacy has yet to be found in humans[125]
R21 VaccineRecombinant protein vaccinesIllicit a higher anti-CSP antibody countErythrocyticPhase I/IIaEfficacy has yet to be found in humans[92]
Pfs 230& Pfs48/45Potential new targetPfs230and Pfs48/45combined with a FAB fragment of a monoclonal antibody, 4F12, can act on parasitic gametes by forming a membrane-bound protein complex and increase the vaccine activityTransmission Blocking VaccineNoneEfficacy has yet to be found in humans[123]
Pfs25Recombinant conjugated vaccinesAntibodies against the Pfs25antigen in the human host to stop the development and transmission of the parasite when the vector feeds on the host.Transmission Blocking VaccinePhase IEfficacy has yet to be found in humans[120]
PfGARPPotential new targetGlutamic acid rich proteinErythrocyticNoneEfficacy has yet to be found in humans[115]
PfRH5-PfCyRPA-PfRipr(RCR) complexPotential new targetInduce strain-transcending neutralizing antibodies against blood-stage P. falciparumErythrocyticPhase I/IIEfficacy has yet to be found in humans[116]

Table 3.

Overview of current vaccines candidates against Plasmodium falciparum.

5.1 Pre-erythrocytic vaccines

Pre-erythrocytic vaccines aim to kill infected hepatocytes and prevent sporozoites from reaching the liver [91]. There are various gene targets currently being investigated and in clinical trials.

5.1.1 RTS,S/AS01E

RTS,S/AS01E is a well-known pre-erythrocytic vaccine that has successfully completed phase III of clinical testing. It is currently distributed by World Health Organization (WHO) in Malawi, Ghana, and Kenya to further investigate vaccine efficacy [92]. RTS,S is a vaccine that targets circumsporozoite proteins (CSP) from P. falciparum. CSP are surface proteins that is important in hepatocyte invasion. Interactions between CSP and heparin sulfate proteoglycans (HSPGs) allows the sporozoite to attach to the surface of hepatocytes and triggers a signaling cascade that allows for the sporozoite to invade liver cells [93]. Subsequent to invasion, the sporozoites will mature, multiply, and feed on the hepatocytes until the hepatocytes lyse and release merozoites into the bloodstream. Preventing the invasion of sporozoites will inhibit the progression and severity of the disease. Using the C-terminus and central tandem repeat (NANP) of PfCSP, Hepatitis B surface membrane antigen (HSbAg), and an AS01 adjuvant system, the vaccine will elicit a strong, stable immune response [94]. After vaccination, the host immune system will response to PfCSPantigen by producing anti-CSP antibodies and activating CD4+ T cells [95]. RTS,S/AS01E is given on a three-dose schedule within three months followed by a fourth dose at 20 months [94]. It has been shown across clinical malarial studies that the vaccine has an 39–50% efficacy in children ages 5–17 months and 23–30% efficacy in children ages 6–12 months [96, 97, 98]. Efficacy warned rapidly from 35.2% and 20.3% to 19.1% and 12.7%, respectively, in children and infants within 20–32 months without a booster [94]. Such a decay in vaccine efficacy could be due to reduced IgG and IgM antibodies against CSP antigen. Anti-CSP antibodies were shown to increase by almost 10-fold from 318.2 EU/mL to 34.2 EU/mL in children one month after a booster was given [92]. Apart from the short-lived nature of the vaccine, older children who were vaccinated showed an increased risk of malarial infections, likely due to RTS,S/AS01E interference with naturally acquired immunity [92]. Another similar vaccine R21 is currently testing in Phase 1/2a clinical trials [99]. This vaccine aims to elicit a high anti-CSP antibody content similar to the mechanisms of RTS,S vaccine. R21 comprises particles from CSP-HBsAg protein infused with an adjuvant, matrix-M [99]. It has been shown to increase the production of T cells and is still in the process of development [92]. Further studies should investigate alternative antigens that can elicit stronger and long-lasting efficacy as well as the mechanisms of the cell-mediated immune response against malaria in humans.

5.1.2 PfSPZ

Plasmodium falciparumsporozoites (PfSPZ) is another pre-erythrocytic vaccine target. As aforementioned, sporozoites transferred from the infected Anopheles mosquito to the human host. They enter the bloodstream and reach the liver before invading the hepatocytes using the sporozoite proteins P36 and P52. P36 interacts with hepatocyte’s extracellular receptor EphA2 to create a protective parasitophorous vacuole that facilitates hepatocyte invasion [100]. PfSPZvaccine prevents the sporozoites reaching the liver and infecting hepatocytes [101], and is currently undergoing phase III clinical trial [102]. PfSPZvaccine was designed to have a live, whole sporozoite that is radiated-attenuated. It is injected intravenously and given in 3–5 doses. Recent studies using controlled human malaria infection (CHMI) showed that this vaccine provided about 33 weeks of stabilized protection in 50% of the vaccinated subjects [103]. The vaccine induced interferon gamma (IFN-γ) that can recruit and activate CD8+ and CD4+ T cells against homologous and heterologous parasitic strains [103]. Subjects who received the PfSPZvaccine also developed IgM antibodies that can help inhibit proliferation of the parasites [104]. However, the vaccine requires specific storage in ultra-cold condition and trained medical workers to inject the vaccine intravenously [92]. Furthermore, efficacy varied by locations. For example, in Mali, 29% efficacy was reported in subject who were exposed to heterologous strain; whereas in CHMI, 83% of subjects were found to be protected from exposure to heterologous strains [102]. Further studies are needed to compare efficacy among different geographical or transmission settings.

5.1.3 PfLSA-1 and PfLSA-3

Liver surface antigen (LSA) is another pre-erythrocytic vaccine target. LSA is essential for the survival of the parasites during the late liver schizogony stage [105]. Schizonts are asexual stage of Plasmodiumthat developed from sporozoites and matured in infected hepatocytes. Once the infected hepatocytes are filled up with mature schizonts, they rupture and release merozoites into the bloodstream to invade erythrocytes. LSA vaccine prevents the maturation of schizonts and rupture of infected hepatocytes. There are two liver stage antigens, LSA-1 and LSA-3, that are used as vaccine targets. PfLSA-1is high conserved in P. falciparumand is found in parasitophorous vacuole in the liver stage of the parasites. PfLSA-1contains 17 amino acids repeats and is associated with the late liver schizont stage [105, 106]. LSA-1 can induce IgG and IgM antibodies as well as CD4+ T cell production [105, 107]. LSA-1 vaccine is currently in phase I clinical trial and is still unclear its efficacy in humans. LSA-3, on the other hand, is found in dense granules in the blood stage of the parasites and the protein is about 175 kDa [108]. LSA-3 appears to play a role in the parasitic growth in infected hepatocytes and erythrocytes [108]. A recent study indicated that LSA-3 provided full protect to chimpanzees from heterologous P. falciparumsporozoites [105]. Like LSA-1, LSA-3 is also in phase I clinical trial and its efficacy and immunogenicity in humans remain unclear.

5.2 Erythrocytic vaccines

Erythrocytic vaccines aim to kill and terminate the asexual reproduction and invasion of the parasite within red blood cells (RBC). Infected individuals typically experience symptoms when the parasites invade a threshold number of RBCs and disrupt their normal functions. Preventing the parasites developed into blood stage will inhibit progression of malaria symptoms such as chills, aches, and fevers.

5.2.1 PfMSP1

Merozoite surface protein 1 (MSP1) is one of the targets used for erythrocytic vaccine. MSP1 is a glycosylphosphatidylinositol-anchored protein found in abundance on the surface of the merozoites [109]. MSP1 plays an important role in the invasion of erythrocytes as it binds and recruits other peripheral merozoite surface proteins to form a complex [109]. MSP1 starts off as a precursor of about 196 kDa and then cleave into four subunits before invading the erythrocytes [110]. The four subunits are held non-covalently forming a complex attached to the merozoite’s GPI anchor [110]. Once the MSP1 complex is formed, it binds with the receptors on erythrocytes and activates a spectrin-binding function to enter the erythrocytes [110]. MSP1 has been shown to elicit both humoral (IgM and IgG antibodies) and cell-mediated immune responses (memory T cells) that lasted about 6 months after immunization [110]. These results are promising as MSP1 vaccine will also activate antibodies for complement fixation, induce opsonizing antibodies, and initiate secretion of reactive oxygen species by other immune cells [110]. To date, MSP1 vaccine is in phase I clinical trial. Further investigation is needed to evaluate efficacy.

5.2.2 PfAMA-1

The erythrocytic vaccine based on Apical Membrane Antigen 1 (AMA1) is currently in phase II clinical trial [111]. The AMA1 protein is approximately 83 kDa and can be found in both the merozoite and sporozoite stages of P. falciparum[111]. The complex AMA1 and another parasite protein namely the rhoptry neck protein 2 (RON2), is essential for merozoite invasion during the blood stage of infection, and initiates the parasite traversal into the RBCs [112]. The AMA1 vaccine has been shown to elicit high levels of antibodies that can block the invasion of the erythrocytes, despite high polymorphisms observed in the AMA1 protein [112]. The AMA1-Diversity Covering (DiCo) vaccine was thus designed to include three recombinant variants of AMA1 and this vaccine is currently testing in phase Ia/Ib clinical trial [113]. To increase efficacy of the AMA1 vaccine, AMA1 was paired with the RON2 receptor and vaccinated in eight Aotusmonkeys [112]. Half of the monkeys were able to achieve complete immunity from the P. falciparuminfection when vaccinated with AMA1 and RON2 [112]. The vaccine with AMA1 and RON2 induced a higher level of antibodies than the AMA1 vaccine. Further investigation is needed to examine other potential AMA1 variants or merozoite structures that can be paired up with the AMA1 protein to increase efficacy.

5.2.3 PfGARP

Plasmodium falciparumglutamic acid rich protein (PfGARP) is an 80 kDa antigen commonly expressed on the surface of infected erythrocytes during the late trophozoite stage [114]. The PfGARPgene is relatively conserved. Antibodies against the PfGARPantigen protein have been shown to confer protection against severe malaria and reduce parasite densities by 3.5 folds [115]. Further, anti-PfGARPantibodies were able to successfully induce apoptosis in ring-stage parasite cultures, resulting in full loss of their mitochondrial function within a 24 hour period [115]. In addition, the size of food vacuoles in the parasites was decreased or condensed tightly around the hemozoin crystals, making them inaccessible and parasite growth was reduced by 76–87% in vitro[115].

5.2.4 PfRH5-PfCyRPA-PfRipr (RCR) complex

The PfRH5-PfCyRPA-PfRipr(RCR) complex is a protein trimer composed of three different proteins PfRH5, PfCyRPA, and PfRiprthat are found on the surface of merozoites [116]. P. falciparumReticulocyte-binding Protein Homolog 5 (PfRH5) is a 63 kDa protein commonly expressed during the schizont stage. After PfRH5binds with basigin (a receptor found on human erythrocytes), a large amount of calcium is released to initiate invasion [116]. Monoclonal antibodies against PfRH5has been found to disrupt the binding between basigin and PfRH5[116]. P. falciparumCysteine-rich Protective Antigen (PfCyRPA) is a highly conserved 43 kDa protein [116]. It plays an important role in erythrocyte invasion by interacting with PfRH5to bind to the receptor basigin [56]. Although PfCyRPAis not immunogenic compared to PfRiprand PfRH5, monoclonal antibodies produced against this protein can cause cross strain neutralization [116]. P. falciparumRH5-interacting Protein (PfRipr) is a highly conserved 120 kDa protein found in the schizont stage [116]. It is composed of 87 cysteines and 10 epidermal growth factor-like (EGF) domains [116]. Prior to erythrocyte invasion, PfRiprcleaves into two different fragments including the N-terminus and C-terminus. The N-terminus contains EGF domains 1 and 2 while the C-terminus contains EGF domains 3–10 [116]. Antibodies against PfRiprEGF domains 6–8 have been shown to neutralize the parasites [116]. Combining the anti-PfCyRPA c12 mAb with anti-RH5 BS1.2 mAbr will inhibit parasite growth in vitrofrom 21–31% to 59%. Thus, this antigen protein complex is expected to elicit a strong immune response against blood stage P. falciparum[117].

5.3 Transmission blocking vaccine (TBV)

TBV aims to prevent and kill the sexual stages of the Plasmodiumparasites before transferring into the mosquito hosts. This vaccine offers protection against infection and transmission.

5.3.1 Pfs25

Pfs25is an important glycophosphatidylinositol-linked protein expressed on the surface of ookinetes. It is found only within the Anopheleshost and is approximately 25 kDa with 11 disulfie bonds [118]. The parasites require Pfs25to survive in the Anopheles’s midgut and develop into oocysts [119]. Pfs25is a conserve protein with low diversity. Pfs25vaccine was designed to elicit antibodies against the Pfs25antigen in humans and prohibit the development and transmission of gametocytes [120]. However, a recent study based on an adjuvant of Pfs25and a non-enveloped virus like protein (VLP) indicated weak IgG antibody responses in healthy individuals [121]. In another study, the antibody response of Pfs25proteins combined with four different adjuvants including alum, Toll-like receptor 4 (TLR-4) agonist glucopyranosal lipid A (GLA) plus alum, squalene–oil-in-water emulsion, and GLA plus squalene–oil-in-water emulsion were compared in mice. Pfs25combined with GLA plus squalene–oil-in-water emulsion was shown to induce the highest amounts of IgG antibodies [122]. Further studies should examine the formulation of this vaccine for better efficacy.

5.3.2 Pfs230 and Pfs48/45

Pfs230and Pfs48/45-based vaccines are antigens rich in cysteine produced by the sexual stage gametocytes [123]. Pfs48/45can be found on the plasma membrane surface of both male and female gametocytes and are bounded to a GPI anchor that form a complex with Pfs230[124]. Pfs230is a 230 kDa protein that contains 14 6-cysteine rich domains [123]. Pfs48/45, on the other hand, contains three 6-cysteine rich domains [124]. The 6-cysteine rich domains of these antigens are essential for the formation of disulfide bonds on epitopes needed for antibody elicitation [124]. A recent study showed that mice injected with fragments of Pfs48/45and Pfs230prodomain produced higher levels of antibodies that induced complement fixation [124]. Pfs230and Pfs48/45combined with a FAB fragment of a monoclonal antibody 4F12 have been shown to further increase vaccine efficacy [123]. This vaccine is currently in early clinical development phase [123, 124].

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6. Conclusion

WHO aims to achieve malaria elimination in at least 35 countries, reduce incidence and mortality rates by 90%, and prevent resurgence in malaria-free countries by 2030. This ambitious goal has been challenged by the emergence and spread of antimalarial resistance, inaccurate diagnostic testing, asymptomatic transmission, and lack of effective vaccines [126]. Information of the Plasmodiumgenomes allow us to improve and reinvent tools/techniques for monitoring parasite changes as well as tracking and stopping transmission of the disease. Several hundreds of P. falciparumgenomes have been generated in the past two decades. Genetic variation and function of various genes have improved our understanding of mutational changes, molecular structure, and evolutionary mechanisms in Plasmodium. There is an urgent need to retrieve utmost biological meaning from the available genomic data and translate such into tools that help resolve epidemiological challenges. This includes the identification of novel antigens for accurate and affordable diagnostic assays and vaccines, informative biomarkers that can distinguish different isolates and pinpoint the source of infections at fine geographical scale, and sensitive tool(s) for large-scale screening of asymptomatic infections in both high and low transmission areas. Future studies should examine how climate/environmental changes and selective pressure from interventions mediate genetic changes in the parasites, how host immune system responses to parasite changes, and how to uncover hidden parasite reservoirs and effectively control transmission.

Acknowledgments

We thank our colleagues at the University of North Carolina at Charlotte and the University of Ghana for the inspiration and discussion that lead to the conceptualization of this paper. We also thank the reviewers for their insightful comments.

Conflict of interest

The authors declare no conflict of interest.

Author contributions

Conceptualization, C.C.D. and E.L.; resources, D.A.J. and E.L.; writing—original draft preparation, C.C.D., C.T.F., J.H., and E.L.; writing—review and editing, C.C.D., C.T.F., L.E.A, Y.A.A., D.A.J., and and E.L.; funding acquisition, E.L. All authors have read and agreed to the published version of the manuscript.

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Funding

This research was funded by NIH/NIAID, grant number R15 AI138002.

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Cheikh Cambel Dieng, Colby T. Ford, Jennifer Huynh, Linda E. Amoah, Yaw A. Afrane, Daniel A. Janies and Eugenia Lo (March 19th 2021). Progress in Parasite Genomics and Its Application to Current Challenges in Malaria Control [Online First], IntechOpen, DOI: 10.5772/intechopen.96530. Available from:

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