Molecular identification of the chitinase genes in Plasmodium relictum
© Garcia-Longoria et al.; licensee BioMed Central Ltd. 2014
Received: 26 February 2014
Accepted: 7 June 2014
Published: 18 June 2014
Malaria parasites need to synthesize chitinase in order to go through the peritrophic membrane, which is created around the mosquito midgut, to complete its life cycle. In mammalian malaria species, the chitinase gene comprises either a large or a short copy. In the avian malaria parasites Plasmodium gallinaceum both copies are present, suggesting that a gene duplication in the ancestor to these extant species preceded the loss of either the long or the short copy in Plasmodium parasites of mammals. Plasmodium gallinaceum is not the most widespread and harmful parasite of birds. This study is the first to search for and identify the chitinase gene in one of the most prevalent avian malaria parasites, Plasmodium relictum.
Both copies of P. gallinaceum chitinase were used as reference sequences for primer design. Different sequences of Plasmodium spp. were used to build the phylogenetic tree of chitinase gene.
The gene encoding for chitinase was identified in isolates of two mitochondrial lineages of P. relictum (SGS1 and GRW4). The chitinase found in these two lineages consists both of the long (PrCHT1) and the short (PrCHT2) copy. The genetic differences found in the long copy of the chitinase gene between SGS1 and GRW4 were higher than the difference observed for the cytochrome b gene.
The identification of both copies in P. relictum sheds light on the phylogenetic relationship of the chitinase gene in the genus Plasmodium. Due to its high variability, the chitinase gene could be used to study the genetic population structure in isolates from different host species and geographic regions.
Malaria parasites have a complicated life cycle that requires several unique adaptive mechanisms that enable the parasite to successfully invade a variety of different tissues both in the vertebrate host and in the arthropod vector. Presumably as a protection against pathogens, arthropods develop a protective peritrophic membrane (PM) around their midgut after each blood meal which remains for 24 hours and then disappears . The PM acts as a barrier blocking the penetration of parasites and not allowing them to spread to other organs . Parasites in turn, have developed three different ways to overcome this barrier by (i) leaving the erythrocytes before the formation of the PM (as is the case Wuchereria infection) , (ii) persisting until the PM disappears (e.g. Leishmania) , or (iii) penetrating the PM (e.g. malaria parasites) . The mechanism which allows malaria parasites to go through the PM of mosquitoes is well described [5–7]. These studies have shown that following the sexual process that takes place in the mosquito stomach, the ookinete has the ability to cross the PM by secreting a chitinase with characteristics of the family 18-glycohydrolases that have catalytic and substrate-binding sites that breaks down this layer [8–10]. After crossing the PM, ookinetes finally transform into oocysts which after maturing (9–11 days ) releases the sporozoites that move to the salivary glands where they are ready for infecting a new host (e.g. birds). Therefore, chitinase secretion has an essential role in the completion of the life cycle of malaria parasites.
The mammalian Plasmodium parasite species have a single copy of the chitinase gene but with two different structures. In the human and primate malaria parasites, Plasmodium vivax and Plasmodium knowlesi and the rodent parasites (Plasmodium berghei, Plasmodium yoelii and Plasmodium chabaudi) the chitinase gene is longer and contains both a catalytic domain and a chitin-binding domain; in contrast, the shorter version present in Plasmodium falciparum and Plasmodium reichenowi lacks the chitin-binding domain . Remarkably, the chicken parasite Plasmodium gallinaceum has functional copies of both the long (PgCHT1) and the short (PgCHT2) chitinase gene  suggesting that it is a common ancestor of the mammalian Plasmodium parasites that subsequently lost either the short or the long copy of the chitinase gene . The phylogenetic relationships among Plasmodium parasites infecting mammals and birds have been intensively debated over the past decades. Some studies have found support for that P. falciparum is more closely related to bird parasites than to the other mammalian malaria parasites [13, 14], whereas other studies support that the mammalian parasites are forming a monophyletic clade [15, 16]. Because P. gallinaceum so far is the only bird malaria parasite investigated for its chitinase genes, it is too early to establish that the occurrence of both chitinase copies is representative for bird malaria parasites in general.
Plasmodium gallinaceum has been the primary model for studies related with chitinase function in avian malaria [1, 17]. However, this species is not the most common malaria parasite in birds. In fact, species belonging to the genus Plasmodium show distinct differences in their distribution and prevalence . The most widespread and harmful avian malaria species is Plasmodium relictum, found to infect more than 70 different bird species, whereas P. gallinaceum has been found to infect only 4 (MalAvi data base 2013-12-02 ). Plasmodium relictum is one of the most generalist malaria parasite in birds and has several mitochondrial cytochrome b lineages (e.g. SGS1, GRW4, GRW11, LZFUS01) that can be found in almost all continents (MalAvi data base 2013-12-02 ). Full understanding of the genetic mechanisms of the infection cycle could help to gain insights into why some parasites are specialist whereas others can infect a large number of different host species.
Despite the wide distribution and harmfulness of P. relictum, no study has tried to determine either if this species has the chitinase gene, nor the number of copies it possesses. Therefore, the objectives of this study were (1) to determine whether the two most widespread lineages of P. relictum (SGS1 and GRW4) have the gene encoding for chitinase, (2) if these lineages have both copies (CHT1 and CHT2) and (3) finally determine the genetic variability of chitinase genes between the lineages SGS1 and GRW4.
Chitinase identification and sequencing
Annealing temperature for all the primers used
Seq (as ordered)
Annealing temp. (°C)
Two samples from previous experimental infections with P. relictum, the cytochrome b lineage SGS1 from crossbills  and GRW04 from great reed warblers , were used as DNA template. Total genomic DNA from the avian blood samples was extracted by standard ammonium acetate protocol . All samples were screened for chitinase using a nested PCR method for chitinase genes with primers as in Table 1. For both steps, PCR reactions were set up in total volumes of 25 μl, containing 15.4 μl of ddH2O, 1.5 μl of MgCl2 (25 mM), 2.5 μl dNTP (10 mM), 2.5 μl 10x Buffer, 1 μl of each primer (10 μM), 0.1 of Taq polymerase and 1 μl of each sample (25 ng DNA/μl). The PCR temperature profile was 95°C for 2 min followed by 25 or 35 cycles of 95°C for 30 sec, annealing temperature according to Table 1 for 30 sec and 72°C for 30 sec and terminated by a step of 72°C for 10 min. For the SGS1 isolate we used an additional set of primers (PgCHT1_F3, PgCHT1_R3, PgCHT2_F3, PgCHT2R4) to amplify a region 3’ to the fragment obtained with the nested protocol. Positive amplifications were precipitated and sequenced using a dye terminator cycling sequencing (big dye) kit and loaded on an ABI PRISM™ 3100 sequencing robot (Applied Biosystems. Florida. USA).
Sequences from P. relictum were aligned with the available chitinase gene sequences from Plasmodium spp. (P. gallinaceum CHT1: AF064079; CHT2: AY842482; P. berghei CHT1: AJ305256; P. yoelii CHT1: AB106898; P. knowlesi CHT1: XM002257469; P. vivax CHT1: AB106896; P. falciparum CHT1: AF127445; P. reichenowi CHT1: AY842483) using Geneious translation alignment tool. The quality of the alignment was checked by manual inspection. The combined phylogenetic tree for the two copies was constructed in the programme MEGA 5.2 and using a Maximum Likelihood model. Bootstrap values were used in order to obtain a consensus phylogeny using 200 iterations.
The nucleotide (and amino acid) distances were compared between P. gallinaceum and P. relictum for both copies using a Pairwise distance matrix. For the long copy a distance of 10.0% was found (9.2%) between SGS1 and P. gallinaceum. For the short copy, a distance of 11.0% (10.6%) was found between SGS1 and P. gallinaceum. Over the regions for which data of P. relictum are available from both isolates of P. relictum, SGS1 and GRW4 differed by 1.5% (0.8%) for the short copy and 4.1% (3.6%) for the long copy.
The chitinase gene can consist of one or two copies , a long and a short one. Previous studies have established that some malaria parasites only have one copy (e.g. P. falciparum[10, 23] and P. berghei) while only P. gallinaceum has both variants . Molecular results showed that P. relictum has both copies encoding for chitinase (PrCHT1 and PrCHT2). Plasmodium relictum is as far as it is known, the second malaria parasite demonstrated to have both copies. As P. gallinaceum and P. relictum are quite distantly related among the Plasmodium parasites infecting birds [15, 16] suggests that the presence of two chitinase gene copies is widespread among the bird Plasmodium parasites. Hence, avian malaria parasites are, to date, the only parasites with both copies. Li et al.  suggested that avian malaria parasites could be the ancestor for the chitinase gene in malaria parasites of primates and rodents. Thus, given the current phylogenetic hypothesis, it can be assumed that mammalian parasites evolved from an avian parasite that carried two copies of the chitinase gene.
The bar-coding gene for molecular identification of Plasmodium parasites of birds is the cytochrome b gene [25–27]. When a genetic difference between lineages exceeds 5% this is often followed by distinct morphological differentiation which allows for identification of morphological defined species . Obviously, differences are lower when lineages within the same morphological defined species are compared. The MalAvi data base  shows that the genetic variability in the cytochrome b between SGS1 and GRW4 is 1.8% (9 nucleotides different in 480 bp). However, the present study shows that the genetic variability between SGS1 and GRW4 in the chitinase gene was much higher, 4.1% (14 different nucleotides in 339 bp). Moreover, the genetic distance in the cytochrome b between P. relictum and P. gallinaceum is 6.9% (29 nucleotides different in 480 bp). The results of this study shows that the genetic distance between P. relictum and P. gallinaceu m in the short copy was 13.1% (44 different nucleotides in 339 bp). Previous studies have identified some nuclear genes with a high variability in P. relictum, for instance the msp1 gene , that can be used for epidemiological studies of the malaria parasite. In the same way, the chitinase gene could be a good candidate and complement for studies of genetic population structure of the parasites.
In conclusion, the present study demonstrates that the most widespread and harmful avian malaria parasite, P. relictum, have the gene encoding for chitinase. In accordance with previous studies on avian malaria (i.e. P. gallinaceum), the present study demonstrates that occurrence of both copies (PrCHT1 and PrCHT2) seems to be widespread across avian Plasmodium species. Additionally, the present study demonstrates that the genetic variability of the chitinase gene was high between the two analysed lineages of P. relictum (SGS1 and GRW4).
To determine the phylogenetic relationship between the chitinase gene in malaria parasites, future studies could search for the number of fragments in other species of haemosporidian parasites and most importantly in the genera closely related to Plasmodium that are transmitted by vectors of other dipteran families than Culicidae. Another interesting approach would be to analyse the chitinase gene in parasites isolated from a wide range of bird species with a high prevalence of P. relictum and different habitat uses, looking at the gene variability in P. relictum.
L. Garcia-Longoria was supported by a PhD grant from Ministry of Economy and Competition of Spain (CGL2009-08976 and CGL2012- 36665). The laboratory work was financially supported by a grant from the Swedish Research Council to S.B. (621-2013-4839).
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