The evolutionary host switches of Polychromophilus: a multi-gene phylogeny of the bat malaria genus suggests a second invasion of mammals by a haemosporidian parasite
© Witsenburg et al; BioMed Central Ltd. 2012
Received: 21 November 2011
Accepted: 22 February 2012
Published: 22 February 2012
The majority of Haemosporida species infect birds or reptiles, but many important genera, including Plasmodium, infect mammals. Dipteran vectors shared by avian, reptilian and mammalian Haemosporida, suggest multiple invasions of Mammalia during haemosporidian evolution; yet, phylogenetic analyses have detected only a single invasion event. Until now, several important mammal-infecting genera have been absent in these analyses. This study focuses on the evolutionary origin of Polychromophilus, a unique malaria genus that only infects bats (Microchiroptera) and is transmitted by bat flies (Nycteribiidae).
Two species of Polychromophilus were obtained from wild bats caught in Switzerland. These were molecularly characterized using four genes (asl, clpc, coI, cytb) from the three different genomes (nucleus, apicoplast, mitochondrion). These data were then combined with data of 60 taxa of Haemosporida available in GenBank. Bayesian inference, maximum likelihood and a range of rooting methods were used to test specific hypotheses concerning the phylogenetic relationships between Polychromophilus and the other haemosporidian genera.
The Polychromophilus melanipherus and Polychromophilus murinus samples show genetically distinct patterns and group according to species. The Bayesian tree topology suggests that the monophyletic clade of Polychromophilus falls within the avian/saurian clade of Plasmodium and directed hypothesis testing confirms the Plasmodium origin.
Polychromophilus' ancestor was most likely a bird- or reptile-infecting Plasmodium before it switched to bats. The invasion of mammals as hosts has, therefore, not been a unique event in the evolutionary history of Haemosporida, despite the suspected costs of adapting to a new host. This was, moreover, accompanied by a switch in dipteran host.
KeywordsPolychromophilus Malaria Haemosporida Chiroptera Plasmodium Host switch Phylogenetic analysis Outgroup selection
Five genera belonging to the order of Haemosporida (Apicomplexa) are known to infect mammals: Plasmodium, Hepatocystis, Polychromophilus, Nycteria and Rayella[1, 2]. The dipteran vectors of the first three haemosporidian genera are represented by Culicidae (Anopheles spp.), Ceratopogonidae and Nycteribiidae respectively, while the vectors of Nycteria and Rayella are unknown [1, 2]. Culicidae and Ceratopogonidae also act as vectors of the avian and saurian Haemosporida [1, 3]. These shared vectors suggest that haemosporidian parasites might have invaded mammals multiple times during their evolution. On the other hand, the switch to mammals is thought to have been an evolutionary demanding process for the parasite  and therefore a rare event .
Molecular phylogenetic studies to date have been able to detect only a single host switching event to mammals: mammalian Plasmodium and Hepatocystis, the main mammal-infecting genera, had a common origin and formed a monophyletic sister clade to sauropsid Plasmodium[6, 7]. However, these phylogenetic studies suffer from incomplete taxon sampling with most investigations including, besides the genera Plasmodium and Hepatocystis, only the avian Haemoproteus and Leucocytozoon. Consequently, with no knowledge of the evolutionary origin of the other mammalian haemosporidian groups (i.e. Rayella, Nycteria, Polychromophilus), a second move into mammals cannot be excluded.
One possible approach for resolving this standing question is to select a haemosporidian genus that could potentially have switched to mammal hosts independently of mammalian Plasmodium/Hepatocystis. A good candidate genus for this is Polychromophilus as it is well described, with the majority of its life cycle well documented, including its vector stage. Moreover, it infects mammals but is not transmitted by Culicidae like Plasmodium, nor Ceratopogonidae like Hepatocystis, but by Nycteribiidae (Diptera: Hippoboscoidea). Furthermore, Polychromophilus' vertebrate host species range is restricted to the insectivorous bats (Microchiroptera). A phylogenetic analysis of Polychromophilus can, therefore, elucidate whether it arose through an independent switch to mammal hosts .
The Nycteribiidae vectors are also known as nycteribids or bat flies. These haematophagous flies are completely adapted to a parasitic lifestyle in the fur of bats in that they have lost their wings, have no or reduced eyes and possess hooking claws which allow them swift movements through the fur [13, 14]. Coradetti  was the first to detect sporozoites in their salivary glands and later studies confirmed his finding [12, 16].
The aim of this study was to test these three hypotheses against each other. Though previous studies on the phylogenetic relationships of Polychromophilus have been done, all used only a single gene. Different genes in a single organism can show different evolutionary patterns and it is, therefore, recommended to use multiple genes for accurate relationship estimation . The four genes from three different genomes sequenced for this study represent two species of Polychromophilus (being the two type species of the two proposed subgenera). These sequences were subsequently combined with an existing dataset of 60 species of Haemosporida to clarify the phylogenetic relationships and gain insight into the evolutionary host switches of Polychromophilus.
Sample collection and preparation
Four Miniopterus schreibersii (Schreibers' bent-winged bat) were caught using mist nets in the entrance of an abandoned mine in western Switzerland under authorization 2203 issued by the Veterinarian Service of Canton Vaud, Switzerland. Blood was obtained by puncturing the uropatagial vein with a 0.5 mm gauge needle (Neolus). The blood beads that consequently formed on the uropatagium (between 10 and 30 μl total) were taken up in a microvette with EDTA (Sarstedt) and stored at 4°C until further analysis. Haemostatic cotton was applied on the punctured vein until the bleeding had stopped before releasing any bats.
One drop of blood was applied to a glass microscope slide for later visual identification of the parasite species. After smearing the blood, the slide was dried and immediately submerged in 100% methanol for fixation. Finally 5% Giemsa-staining was applied for one hour to stain the cells. DNA was extracted from whole blood using the DNeasy Blood and Tissue kit (Qiagen). Megali et al.  provided extracted DNA samples from blood of Myotis daubentoni (Daubenton's bat) which contained P. murinus infections. These infections were previously shown to be characterized by different cytochrome b haplotypes .
For the phylogenetic reconstruction, four genes were selected from the three cellular genomes: two mitochondrial DNA sequences, cytochrome b (cytb, 607 bp) and cytochrome oxidase subunit I (coI, 768 bp); one DNA sequence from the apicoplast, caseinolytic protease C (clpc, 502 bp); and one nuclear DNA sequence, adenylosuccinate lyase (asl, 186 bp).
Name, sequence and PCR conditions of the primers used
47°C, 30 s
72°C, 50 s
50°C, 30 s
72°C, 30 s
50°C, 30 s
72°C, 50 s
48°C, 30 s
72°C, 30 s
57°C, 30 s
72°C, 50 s
62°C, 30 s
72°C, 50 s
55°C, 30 s
72°C, 50 s
55°C, 30 s
72°C, 50 s
All successfully amplified samples were purified according to the manufacturer's protocol using the Wizard PCR Clean-Up system (Promega) or the Minelute PCR Purification kit (Qiagen) in the case of asl. DNA concentrations were estimated by visualization on a 1.5% agarose gel with a 100 bp reference ladder (Roche). For the sequencing reactions ~20 ng of purified PCR product, 2 μl Big Dye Terminator v3.1 and 1 μl of 10 mM primer were mixed to a 10 μl volume. Sequence analysis was performed on an ABI Prism 3,100 genetic analyser (Applied Biosystems). Sequence chromatographs were checked for ambiguities with Chromas Lite v2.01 (Technelysium).
The obtained sequence data were combined with the same gene sequences of 60 other haemosporidian species obtained from GenBank (see Additional file 1). These 60 species represent the major clades of the Haemosporida, i.e. Leucocytozoon, Haemoproteus (Haemoproteus), Haemoproteus (Parahaemoproteus), Hepatocystis and Plasmodium (including mammalian, avian and saurian). Sequences were aligned with ClustalW as implemented in MEGA version 5 . The single-gene alignments were concatenated using FASconCAT .
All phylogenetic reconstructions were done using both Maximum Likelihood (ML) analysis and Bayesian inference (BI). For ML analysis, the PhyML software  was used for the single-gene alignments. Since PhyML does not allow for partitioning of the data RAxML  was used for the concatenated alignment. Models of nucleotide substitution were GTR + Γ + I for cytb, co1 and clpc and GTR + Γ for asl, as determined by MrAIC . For each analysis, the transition rates of the GTR model, the shape of the Γ-distribution and the proportion of invariable sites were estimated by the program. Both the RAxML and PhyML analyses were assessed by performing 1,000 bootstrap replicates.
For the Bayesian analysis, the same models of character evolution as described for the ML analyses were implemented with MrBayes 3.1.2 . In the concatenated analysis the data were again partitioned by gene, where each partition had its corresponding model and independent parameter estimations. The MCMC algorithm was done with four chains and was run for 20,000,000 generations, sampling every 1,000 generations. Two independent runs were performed to assess convergence to the correct posterior distribution. All parameters were checked for convergence using Tracer v1.5 and the first 10% of samples of each run was discarded as burn-in. All computations were performed on the Vital-IT cluster of the Swiss Institute of Bioinformatics.
Rooting the tree
Which outgroup to use has been a matter of debate lately. Perkins and Schall  identified Leucocytozoon as the most primitive clade of the order, using Theileria as an outgroup in their analysis of cytb sequences. But a recent study by Outlaw and Ricklefs  demonstrated that, when using a relaxed molecular clock, Leucocytozoon becomes the most derived group, effectively turning the tree inside-out. The authors argue that most ancient divergence should be between the mammal-infecting Plasmodium and Hepatocystis on the one side, and avian/saurian Plasmodium, both subgenera of Haemoproteus and Leucocytozoon on the other.
For the phylogenetic tree reconstructions, the Leucocytozoon spp. were initially selected as the outgroup, but these results were tested for their robustness by redoing the analyses using different rooting methods: 1) forcing the mammalian Plasmodium/Hepatocystis clade as outgroup instead of Leucocytozoon; 2) adding amino acid sequences of the more distantly related Babesia spp. as the outgroup (see Additional file 1) and repeating the ML analyses; 3) using the molecular clock methods similar to Outlaw and Ricklefs  but with varying priors: a Yule or birth-death tree prior, a strict, a log-normal relaxed or an exponential relaxed clock with a GTR + Γ + I substitution model, 20 million generations sampling every 2,000 generations and two independent MCMC runs using BEAST [27–29].
The Kishino-Hasegawa topological test results
Single gene tree
Concatenated 4 genes tree
For each of the three hypotheses on the Polychromophilus origin a corresponding topology was constructed. This was done by restricting the placing of Polychromophilus during tree reconstruction in RAxML, forcing it either with the mammal-infecting Plasmodium/Hepatocystis clade (hypothesis 1), the Haemoproteus (Haemoproteus) clade (hypothesis 2) or with the sauropsid Plasmodium clade (hypothesis 3). These restricted topologies were then tested together with the topology produced by the maximum likelihood analysis using a Shimodaira-Hasegawa test  as implemented in PAML 4 .
The haplotypes and corresponding accession numbers for GenBank per sequenced sample per gene
None of the topologies obtained by independent analyses of the separate genes conflicted with the topology resulting from the concatenated alignment (Kishino-Hasegawa tests: cytb: Δlnl = 2.8, pKH = 0.432, coI: Δlnl = 12.1, pKH = 0.234, clpc: Δlnl = 9.3, pKH = 0.270), except for asl (Δlnl = 81.0, pKH < 0.001). Despite this strong rejection, both the ML and BI trees of asl had only few supported nodes and only closely related pairs were recovered (data not shown). A possible cause of the incongruence detected could be positive selection events in the evolution of the asl nuclear sequence . However, analyses performed with Codeml  did not show signs of positive selection on the nuclear gene.
Although the reasons for this DNA region to be rejected by the topology tests are unclear, the length of the asl gene fragment sequenced in this study is very small (186 bp). This could suggest that random errors are responsible for creating the incongruences observed with this gene. Adding other, and especially longer, nuclear genes would certainly bring more information to test if the evolutionary relationships estimated from the different genomes are congruent or if specific gene trees best represent the evolution of each DNA regions. Different cellular genomes often have different evolutionary histories; even within a single genome not all genes show the same phylogenetic relationships .
Diversity of Polychromophilus species
Polychromophilus forms its own clearly defined clade in both the BI and ML reconstructions. Within this clade, the two species of Polychromophilus form well supported separate sister clades (see Figure 3). The distinction between P. melanipherus and P. murinus has often been made based on host species, since P. melanipherus was by definition confined to Miniopterus schreibersii as hosts. This distinction, however, has been qualified as 'arbitrary' and 'unsatisfactory' . This study demonstrates for the first time that there is a clear genetic distinction between the two Polychromophilus species, confirming their taxonomic status of different species from a molecular point of view.
However, to determine whether this level of genetic divergence between P. murinus and P. melanipherus merits their placement in different subgenera  or even different genera , other species of the genus should be added (e.g. P. deanei and P. adami). Without these supplementary species, the overall observed genetic diversity within the genus Polychromophilus is low; it is clearly less than that of the genera Plasmodium and Haemoproteus or even less than the diversity found in subgenera like P. (Vinckeia) and H. (Parahaemoproteus). No critical level of genetic diversity exists as a precondition for the elevation of a subgenus, but the low diversity found within Polychromophilus does suggest that confirming P. (Bioccala) as a separate genus would cause a taxonomic asymmetry within the Haemosporida.
Two more haemosporidian genera infecting bats have been described: Dionisia and Biguetiella. Both contain only a single species and are described as 'little different' from Polychromophilus (Polychromophilus) and as 'a vicariant form of' Polychromophilus (Bioccala), respectively. Whether their similarities to Polychromophilus spp. are because of convergence or shared ancestry can only be tested by combining the morphological data with molecular methods . A big obstacle in studying these unfamiliar species however is the lack of observations. No other records of Biguetiella or Dionisia exist. Single descriptions of new parasite species found in a limited number of hosts are a problem encountered more often by parasitologists and can severely hamper classification .
Polychromophilus' placement in the phylogeny of Haemosporida
The Shimodaira-Hasegawa topological test results comparing the three hypothetical topologies
Best tree (hypothesis 3)
It is less clear where within the Plasmodium clade Polychromophilus belongs. Neither phylogenetic method indicates that Polychromophilus originated from mammalian Plasmodium/Hepatocystis and both instead produced topologies suggesting a sauropsid origin (see Figure 3). However, the actual support for the node separating the mammalian clade from sauropsid Plasmodium/Polychromophilus clade is low. The BI supports the monophyly of sauropsid Plasmodium and Polychromophilus (hypothesis 3) with a posterior probability of 0.92, but the ML support of that same critical node is absent (bootstrap value of 40/100). The topological test comparing the different phylogenetic scenarios did not provide more support for either hypothesis 1 or 3 (see Table 4).
Most of the alternative rooting methods favour hypothesis 3. Indeed, rooting the tree with the mammalian Plasmodium clade instead of Leucocytozoon, as suggested by Outlaw and Ricklefs , validates the conclusion of a sauropsid origin of Polychromophilus in both BI and ML (see Additional file 2).
The choice of the prior distributions guiding either the distribution of mutation rates across the tree (log-normal vs exponential) or the divergence times (Yule vs birth-death) does not change the conclusion. All the molecular clock analyses place Polychromophilus within the sauropsid Plasmodium clade, with clade credibilities between 0.87 and 1. However the root itself does change depending on the prior set. The Yule and log-normal prior lead to the placement of the Leucocytozoon as the outgroup, whereas the mammalian Plasmodium/Hepatocystis clade is placed as the outgroup with the birth-death tree and exponential relaxed clock (see Additional file 2).
The ML analysis using Babesia as an outgroup produces a topology with very little support. All major nodes have bootstrap values of < 50/100, so no outgroup can be identified, nor can Polychromophilus be placed within the tree with any confidence (see Additional file 3). The genetic divergence between Babesia (Piroplasmida) and the Haemosporida is very high, which results in a very long branch leading to the Babesia lineages. This changes the rooting procedure to a problem of 'long-branch attraction' with all corresponding biases , and these analyses should therefore be approached with caution .
None of the used phylogenetic methods reject our third hypothesis, stating that Polychromophilus is monophyletic with the sauropsid Plasmodium clade. ML and the topological test could not discriminate between hypothesis 2 and 3, but BI and molecular clock rooting methods gave more support for the latter hypothesis. These analyses are far from conclusive, but do suggest that Polychromophilus did not evolve from a mammal-infecting ancestor, but has instead invaded the mammalian class of hosts independently.
Our results show that the three DNA regions used in the combined matrix do not provide sufficient phylogenetic information to unambiguously place the Polychromophilus lineage. When combining regions from different genomes, this could introduce sufficient conflict to reduce the confidence in the reconstructed trees, even if the topology tests did not identified major incongruence. The way forward to clearly place the Polychromophilus lineage within the large Plasmodium clade is to sequence longer stretches of DNA regions, in particular from the nuclear genome, and to use gene tree approaches to identify the best evolutionary relationships at the species level [39, 40].
The close relation between Polychromophilus and avian Haemosporida has been suggested before. Carreno et al.  produced a phylogeny based on life-history and ultra-structure characters and concluded that Polychromophilus is most closely related to Haemoproteus, a hypothesis rejected by the current study. Megali et al.  used a 705 bp cytb fragment and concluded that Polychromophilus shared its closest common ancestry with avian Plasmodium. However, the base of their tree was not well resolved. The authors themselves recommended the use of multiple genes.
Duval et al.  discussed bat Haemosporida, but never identified the species. However, their molecular analyses, again using only cytb, grouped their samples clearly with sauropsid Plasmodium, leading to a similar conclusion as the current study. In their paper, they cautiously did not name their collected species. However, the corresponding sequences that are available in GenBank have been identified as 'Hepatocystis sp.'. Based on the work of Megali et al.  it is very likely that part of those sequences are actually Polychromophilus species. Misidentification is a big obstacle in apicomplexan research as a whole  and haemosporidian research in particular . Therefore, caution is required when naming species for GenBank.
Switch of host, switch of vector
Parasitizing a new, mammalian host likely necessitated many adaptive changes, given their characteristic, non-nucleated red blood cells. The cytb DNA region sequenced here showed long branches of non-synonymous substitutions separating the avian from the mammal clade . Many lineages have become extinct over time during the evolution towards the mammalian and avian Plasmodium lineages . Nevertheless Polychromophilus' origin suggests that the switch to mammalian hosts happened at least twice during Haemosporida evolution. Rayella is thought to have originated from Hepatocystis and has been classified as such , but Nycteria's origins are more elusive; whether it is a case of yet another independent host switch, or an ancient mammalian Plasmodium lineage that has survived the pruning on that branch, remains to be investigated.
Haematophagy has appeared multiple times in the evolution of the Diptera. It evolved once at the origin of the superfamily Hippoboscoidea and is shared by all its members . Consequently, many Hippoboscoidea spp. are implicated in the transmission of diseases, most notably sleeping sickness (Glossinidae) and malaria (Hippoboscidae and Nycteribiidae). The relatively high relatedness of the latter two families  is not reflected by their haemosporidian parasites. This study convincingly rejected the hypothesis that hippoboscid-transmitted H. (Haemoproteus) shares its most recent common ancestor with the nycteribid-transmitted Polychromophilus. A cospeciation event of these Haemosporida with their dipteran hosts can, therefore, clearly be excluded.
Instead, Polychromophilus' ancestor must have been vectored by of a member of the Culicidae, as are all modern Plasmodium species. Culicidae are one of the oldest members of the Diptera, an order with a higher radiation of species than all terrestrial vertebrates put together . The phylogenetic distance between Culicidae and Nycteribiidae is one of the largest within the order , yet the adaptations required for this new vector were seemingly acquired in parallel to those required for the new mammalian host.
Because the Nycteribiidae are completely specialised to bats, the first appearance of Polychromophilus in bats must have been mediated by either mosquitoes or via the hippoboscid flies. Many Culicidae spp. feed on both mammals and birds readily, and within the Hippoboscidae, the host switch from mammals to birds has happened several times . Therefore, both could have been responsible for the first transmission. However, once Polychromophilus' ancestor was introduced in bats, adapting to the nycteribid vectors likely had large fitness advantages. Specifically, the haematophagous lifestyle of both males and females combined with their high prevalence on bats , and ease of moving between bat-hosts (unpublished observations), make the Nycteribiidae an ideal vector for the protozoan parasite. However, this same switch to Nycteribiidae also limited the potential range of Polychromophilus vertebrate hosts to the Chiroptera.
The phylogenetic reconstruction of three genes of Polychromophilus spp. demonstrates that the P. melanipherus and P. murinus are clearly two genetically distinct species. Only the addition of the other Polychromophilus spp. can validate the current division of Polychromophilus in separate subgenera. Polychromophilus is clearly not related to Haemoproteus (Haemoproteus). Instead Bayesian inference and molecular clock outgroup free phylogenetic reconstructions suggest that the Polychromophilus most likely had a bird- or reptile-infecting Plasmodium ancestor. The switch to mammalian hosts would, therefore, not have occurred once, but at least twice in the haemosporidian evolutionary past. This event was accompanied by the adaptation to a new, phylogenetically distant dipteran vector.
We would like to give a big thank you to Anne-Lyse Ducrest and Céline Simon for advice on and assistance with the molecular work. We would also like to give our gratitude to Emily Clark and two anonymous referees for helpful comments improving this manuscript. We thank the Swiss Institute of Bioinformatics for their support and the availability of the Vital-IT facilities. This research was supported by grant 31003A_120479 from the Swiss National Science Foundation.
- Garnham PCC: Malaria Parasites and Other Haemosporidia. 1966, Oxford: Blackwell Scientific Publications, 1Google Scholar
- Dasgupta B: A new malarial parasite of the flying squirrel. Parasitology. 1967, 57: 467-474. 10.1017/S0031182000072358.View ArticlePubMedGoogle Scholar
- Valkiũnas G: Avian Malaria Parasites and Other Haemosporidia. 2005, Boca Raton: CRC Press, EnglishthGoogle Scholar
- Outlaw DC, Ricklefs RE: Comparative gene evolution in haemosporidian (Apicomplexa) parasites of birds and mammals. Mol Biol Evol. 2010, 27: 537-542. 10.1093/molbev/msp283.View ArticlePubMedGoogle Scholar
- Yotoko KSC, Elisei C: Malaria parasites (Apicomplexa, Haematozoea) and their relationships with their hosts: is there an evolutionary cost for the specialization?. J Zool Syst Evol Res. 2006, 44: 265-273. 10.1111/j.1439-0469.2006.00377.x.View ArticleGoogle Scholar
- Martinsen ES, Perkins SL, Schall JJ: A three-genome phylogeny of malaria parasites (Plasmodium and closely related genera): evolution of life-history traits and host switches. Mol Phylogenet Evol. 2008, 47: 261-273. 10.1016/j.ympev.2007.11.012.View ArticlePubMedGoogle Scholar
- Perkins SL, Schall JJ: A molecular phylogeny of malarial parasites recovered from cytochrome b gene sequences. J Parasitol. 2002, 88: 972-978.View ArticlePubMedGoogle Scholar
- Carreno RA, Kissinger JC, McCutchan TF, Barta JR: Phylogenetic analysis of haemosporinid parasites (Apicomplexa: Haemosporina) and their coevolution with vectors and intermediate hosts. Arch Protistenkd. 1997, 148: 245-252. 10.1016/S0003-9365(97)80005-X.View ArticleGoogle Scholar
- Garnham PCC: The zoogeography of Polychromophilus. Ann Parasitol Hum Comp. 1973, 48: 231-242.PubMedGoogle Scholar
- Landau I, Rosin G, Miltgen F, Hugot JP, Leger N, Beveridge I, Baccam D: Sur le genre Polychromophilus (Haemoproteidae, parasite de microchiroptères). Ann Parasitol Hum Comp. 1980, 55: 13-32.Google Scholar
- Landau I, Baccam D, Ratanaworabhan N, Yenbutra S, Boulard Y, Chabaud AG: Nouveaux Haemoproteidae parasites de chiroptères en Thailande. Ann Parasitol Hum Comp. 1984, 59: 437-447.PubMedGoogle Scholar
- Gardner RA, Molyneux DH: Polychromophilus murinus: a malarial parasite of bats: life-history and ultrastructural studies. Parasitology. 1988, 96: 591-605. 10.1017/S0031182000080215.View ArticlePubMedGoogle Scholar
- Dick CW, Patterson BD: Bat flies: obligate ectoparasites of bats. Micromammals and Macroparasites: From Evolutionary Ecology to Management. Edited by: Morand S, Krasnov BR, Poulin R. 2006, Tokyo: Springer-Verlag, 179-194.View ArticleGoogle Scholar
- Theodor O: An Illustrated Catalogue of the Rothschild Collection of Nycteribiidae. 1967, London: British Museum (Natural History)Google Scholar
- Corradetti A: Alcuni protozoi parassiti di Nycteribiidae del genere Listropoda. Ann Igiene. 1936, 46: 444-460.Google Scholar
- Mer GG, Goldblum N: A haemosporidian of bats. Nature. 1947, 159: 444-444.View ArticlePubMedGoogle Scholar
- Petersen FT, Meier R, Kutty SN, Wiegmann BM: The phylogeny and evolution of host choice in the Hippoboscoidea (Diptera) as reconstructed using four molecular markers. Mol Phylogenet Evol. 2007, 45: 111-122. 10.1016/j.ympev.2007.04.023.View ArticlePubMedGoogle Scholar
- Megali A, Yannic G, Christe P: Disease in the dark: molecular characterization of Polychromophilus murinus in temperate zone bats revealed a worldwide distribution of this malaria-like disease. Mol Ecol. 2011, 20: 1039-1048. 10.1111/j.1365-294X.2010.04905.x.View ArticlePubMedGoogle Scholar
- Outlaw DC, Ricklefs RE: Rerooting the evolutionary tree of malaria parasites. Proc Natl Acad Sci USA. 2011, 108: 13183-13187. 10.1073/pnas.1109153108.PubMed CentralView ArticlePubMedGoogle Scholar
- Cummings MP, Meyer A: Magic bullets and golden rules: data sampling in molecular phylogenetics. Zoology (Jena). 2005, 108: 329-336. 10.1016/j.zool.2005.09.006.View ArticleGoogle Scholar
- Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S: MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol. 2011, 28: 2731-2739. 10.1093/molbev/msr121.PubMed CentralView ArticlePubMedGoogle Scholar
- Kück P, Meusemann K: FASconCAT, version 1.0. Zool. Edited by: Forschungsmuseum A. 2010, Koenig, GermanyGoogle Scholar
- Guindon S, Gascuel O: A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. Syst Biol. 2003, 52: 696-704. 10.1080/10635150390235520.View ArticlePubMedGoogle Scholar
- Stamatakis A: RAxML-VI-HPC: maximum likelihood-based phylogenetic analyses with thousands of taxa and mixed models. Bioinformatics. 2006, 22: 2688-2690. 10.1093/bioinformatics/btl446.View ArticlePubMedGoogle Scholar
- Nylander JAA: MrAIC.pl. Uppsala. Program Distributed by the Author. 2004, Evolutionary Biology Centre, Uppsala UniversityGoogle Scholar
- Ronquist F, Huelsenbeck JP: MrBayes 3: Bayesian phylogenetic inference under mixed models. Bioinformatics. 2003, 19: 1572-1574. 10.1093/bioinformatics/btg180.View ArticlePubMedGoogle Scholar
- Drummond AJ, Ho SYW, Phillips MJ, Rambaut A: Relaxed phylogenetics and dating with confidence. PLoS Biol. 2006, 4: 699-710.View ArticleGoogle Scholar
- Drummond AJ, Nicholls GK, Rodrigo AG, Solomon W: Estimating mutation parameters, population history and genealogy simultaneously from temporally spaced sequence data. Genetics. 2002, 161: 1307-1320.PubMed CentralPubMedGoogle Scholar
- Drummond AJ, Rambaut A: BEAST: Bayesian evolutionary analysis by sampling trees. BMC Evol Biol. 2007, 7: 214-10.1186/1471-2148-7-214.PubMed CentralView ArticlePubMedGoogle Scholar
- Kishino H, Hasegawa M: Evaluation of the maximum-likelihood estimate of the evolutionary tree topologies from DNA-sequence data, and the branching order in Hominoidea. J Mol Evol. 1989, 29: 170-179. 10.1007/BF02100115.View ArticlePubMedGoogle Scholar
- Jobb G: TREEFINDER. 2008, Munich, Germany: Distributed by the author, October 2008 edition, [http://www.treefinder.de/]Google Scholar
- Shimodaira H, Hasegawa M: Multiple comparisons of log-likelihoods with applications to phylogenetic inference. Mol Biol Evol. 1999, 16: 1114-1116. 10.1093/oxfordjournals.molbev.a026201.View ArticleGoogle Scholar
- Yang ZH: PAML 4: phylogenetic analysis by maximum likelihood. Mol Biol Evol. 2007, 24: 1586-1591. 10.1093/molbev/msm088.View ArticlePubMedGoogle Scholar
- Christin P-A, Besnard G, Edwards EJ, Salamin N: Effect of genetic convergence on phylogenetic inference. Mol Phylogenet Evol.Google Scholar
- Garnham PCC, Lainson R, Shaw JJ: A contribution to the study of Haematozoon parasites of bats - a new Haemoproteid, Polychromophilus deanei n. sp. Mem Inst Oswaldo Cruz. 1971, 69: 119-125. 10.1590/S0074-02761971000100009.View ArticlePubMedGoogle Scholar
- Landau I, Chabaud AG, Miltgen F, Baccam D: Dionisia bunoi n. gen. n. sp. Haemoproteidae parasite du microchiroptère Hipposideros cyclops au Gabon. Ann Parasitol Hum Comp. 1980, 55: 271-280.PubMedGoogle Scholar
- Perkins SL, Martinsen ES, Falk BG: Do molecules matter more than morphology? Promises and pitfalls in parasites. Parasitology. 2011, 138: 1664-1674. 10.1017/S0031182011000679.View ArticlePubMedGoogle Scholar
- Sanderson MJ, Shaffer HB: Troubleshooting molecular phylogenetic analyses. Annu Rev Ecol Syst. 2002, 33: 49-72. 10.1146/annurev.ecolsys.33.010802.150509.View ArticleGoogle Scholar
- Ane C, Larget B, Baum DA, Smith SD, Rokas A: Bayesian estimation of concordance among gene trees. Mol Biol Evol. 2007, 24: 412-426.View ArticlePubMedGoogle Scholar
- Heled J, Drummond AJ: Bayesian inference of species trees from multilocus data. Mol Biol Evol. 2010, 27: 570-580. 10.1093/molbev/msp274.PubMed CentralView ArticlePubMedGoogle Scholar
- Duval L, Robert V, Csorba G, Hassanin A, Randrianarivelojosia M, Walston J, Nhim T, Goodman SM, Ariey F: Multiple host-switching of Haemosporidia parasites in bats. Malar J. 2007, 6: 157-10.1186/1475-2875-6-157.PubMed CentralView ArticlePubMedGoogle Scholar
- Morrison DA: Evolution of the Apicomplexa: where are we now?. Trends Parasitol. 2009, 25: 375-382. 10.1016/j.pt.2009.05.010.View ArticlePubMedGoogle Scholar
- Valkiũnas G, Atkinson CT, Bensch S, Sehgal RNM, Ricklefs RE: Parasite misidentifications in GenBank: how to minimize their number?. Trends Parasitol. 2008, 24: 247-248. 10.1016/j.pt.2008.03.004.View ArticlePubMedGoogle Scholar
- Ricklefs RE, Outlaw DC: A molecular clock for malaria parasites. Science. 2010, 329: 226-229. 10.1126/science.1188954.View ArticlePubMedGoogle Scholar
- Mattingly PF: The paleogeography of mosquito-borne disease. Biol J Linn Soc Lond. 1983, 19: 26-View ArticleGoogle Scholar
- Wiegmann BM, Trautwein MD, Winkler IS, Barr NB, Kim JW, Lambkin C, Bertone MA, Cassel BK, Bayless KM, Heimberg AM, Wheeler BM, Peterson KJ, Pape T, Sinclair BJ, Skevington JH, Blagoderov V, Caravas J, Kutty SN, Schmidt-Ott U, Kampmeier GE, Thompson FC, Grimaldi DA, Beckenbach AT, Courtney GW, Friedrich M, Meier R, Yeates DK: Episodic radiations in the fly tree of life. Proc Natl Acad Sci USA. 2011, 108: 5690-5695. 10.1073/pnas.1012675108.PubMed CentralView ArticlePubMedGoogle Scholar
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