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57 results for “haemosporidian parasites”
Data for article "Haemosporidian parasites (Apicomplexa, Haemosporida) of breeding Common Starling (Sturnus vulgaris) in Latvia"
<p><span>The archive contains data file to reproduce the results presented in the paper “Haemosporidian parasites (Apicomplexa, Haemosporida) of breeding Common Starling (Sturnus vulgaris) in Latvia” published in Wildlife Biology. Age codes of individual birds within the csv file are given according to EURING.</span></p>
Fig. 1 in High prevalence of haemosporidian parasites in Eurasian jays
Fig. 1 Median-joining network of mitochondrial cytochrome b lineages (476 bp, n = 60 sequences) of haemosporidian parasites found in Eurasian jays Garrulus glandarius. Circle size is proportional to the lineage frequency. Lineage names are noted at the associated circles together with one exemplary GenBank association number in parentheses. One hatch mark represents one mutation. Sample origins are represented by different colours, 'MalAvi' referring to sequences from other studies deposited in the MalAvi database (MalAvi 2023). Morphospecies names for GAGLA07 (H. homopicae) and TURDUS2 (H. minutus) are not provided within the figure
Fig. 3 in Haemosporidian parasite infections in grouse and ptarmigan: Prevalence and genetic diversity of blood parasites in resident Alaskan birds
Fig. 3. Bayesian phylogenetic tree of haemosporidian mtDNA cytochrome b haplotypes isolated from Alaskan grouse and ptarmigan species. Node tips are labeled with abbreviation for parasite genus (Haem = Haemoproteus, Leuc = Leucocytozoon, and Plas = Plasmodium), followed by the lineage name, GenBank accession number for each lineage, and avian (Phas = Phasianidae, Anat = Anatiade, Turd = Turdidae, Paru = Parulidae, Scol = Scolopacidae, Embe = Emberizidae, and Frin = Fringillidae) or invertebrate (Simu = Simuliidae) host family. All haplotypes identified in this study are highlighted in red and asterisks following tip labels indicate a lineage that was isolated from Alaskan bird hosts. Numbers on branches indicate posterior probabilities from our analysis. All reference sequences were obtained from the National Center for Biotechnology Information website or the MalAvi database. (For interpretation of the references to colour in this figure legend, the reader is referred to the web version of this article.)
Fig. 2. Minimum spanning network for haemosporidian mtDNA cytochrome b in Haemosporidian parasite infections in grouse and ptarmigan: Prevalence and genetic diversity of blood parasites in resident Alaskan birds
Fig. 2. Minimum spanning network for haemosporidian mtDNA cytochrome b haplotypes isolated from Alaskan grouse and ptarmigan species. Dark circles represent un-sampled nodes. All circles are proportional to the frequency at which the haplotypes were detected. Lines between nodes are drawn to scale based on the number of nucleotide mutations unless otherwise indicated by hash marks.
Fig. 1 in Haemosporidian parasite infections in grouse and ptarmigan: Prevalence and genetic diversity of blood parasites in resident Alaskan birds
Fig. 1. Map of Alaskan sampling regions assembled from multiple game management units and sub-units. Regions were grouped for analysis of haemosporidian prevalence as follows: southcoastal (Kenai Peninsula and southeastern Alaska; GMUs 1C, 1D, 2, 7, 15A, 15B, and 15C), southcentral (Anchorage area and Matanuska-Susitna Valley; GMUs 13A, 13D, 14A, 14C, 16A, and 16B), southwestern (Bristol Bay, Alaska Peninsula, and eastern Aleutian islands; 9D, 9E, and 17C), southern interior (south side of Alaska Range; GMUs 12, 13B, and 13E), northern interior (north side of Alaska Range; GMUs 20A-20E and 25C), and Seward Peninsula (GMU 22C).
Fig. 3 in Detection of haemosporidian parasites in wild and domestic birds in northern and central provinces of Iran: Introduction of new lineages and hosts
Fig. 3. Median joining haplotype network of Haemoproteus lineages. Detected sequences in this study are in bold.
Fig. 2. Bayesian tree reconstructed using 478 in Detection of haemosporidian parasites in wild and domestic birds in northern and central provinces of Iran: Introduction of new lineages and hosts
Fig. 2. Bayesian tree reconstructed using 478-bp mitochondrial cytb gene for avian blood parasites lineages. The amplified sequences in the current study are highlighted in bold. Posterior probability support of>0.8 is displayed for each branch. Schematic tree is summarized in section A and separated clade for each genus is given in sections of B (Plasmodium), C (Haemoproteus), and D (Leucocytozoon).
Fig. 4 in Mosquito identification and haemosporidian parasites detection in the enclosure of the African penguins (Spheniscus demersus) at the SANBI zoological garden
Fig. 4. Maximum likelihood tree showing the clustering of Leucocytozoon sp. (Clade I) and Plasmodium sp. (Clade II) with Haemoproteus sp. as outgroup. Sequences from this study are highlighted with red circles. (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 3. Maximum likelihood tree for Culex species showing the 5 clades representing 5 subgroups. Clade I in Mosquito identification and haemosporidian parasites detection in the enclosure of the African penguins (Spheniscus demersus) at the SANBI zoological garden
Fig. 3. Maximum likelihood tree for Culex species showing the 5 clades representing 5 subgroups. Clade I is the Trifilatus Subgroup (Mattingly and Rageau, 1958) for Cx. torrentium; Clade II and III are the Pipiens Complex; Clade IV the Theileri Subgroup (Sirivanakarn, 1976) for Cx. theileri; and Clade V is the Tarsalis (Edwards, 1932) for Cx. declaratory and Apicinus Subgroups (Edwards, 1932) for Cx. mollis. Lutzia sp. used as outgroups. Sequences from this study are indicated by asterisks (*).
Fig. 1 in Mosquito identification and haemosporidian parasites detection in the enclosure of the African penguins (Spheniscus demersus) at the SANBI zoological garden
Fig. 1. Map of South Africa showing the National Zoological Gardens (NZG). The red star indicates where the African penguin enclosure is located and where mosquito samples were collected (Labuschagne et al., 2008). (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 2. Predicted probabilities and 95 in Is it best on the nest? Effects of avian life-history on haemosporidian parasitism
Fig. 2. Predicted probabilities and 95% confidence intervals of haemosporidian parasitism (Plasmodium, Haemoproteus, and Leucocytozoon). Expected prevalence illustrated according to haemosporidia genera; Plasmodium represented with "P" (a), Haemoproteus represented with "H" (b–c), Leucocytozoon represented with "L" (d–f). Note that in some instances symbol size exceeded the range of confidence intervals.
Fig. 7 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 7. Phylogenetic (ML) relationship of the Polychromophilus cytb gene fragment (378 bp) found in this study (taxa with green circles) and the other global isolates. Polychromophilus isolated from T. melanopogon is placed in the same clade with African bat isolates of P. melanipherus in clade 1. Polychromophilus isolated from My. siligorensis shares the same clade with European bat isolates of P. murinus in clade 2. BS values greater than 50% are shown in the figure. The other clades, consisting of Hepatocystis, Nycteria, Plasmodium, and outgroup are collapsed. (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 5 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 5. Phylogenetic (ML) relationship of the Hepatocystis cytb gene fragment (378 bp) in the present study (taxa with red circles) and the other global isolates from the GenBank™ database. Clade (number) and subclade (letter) are indicated. Haplotype 10 of Hepatocystis in the current study originated from the frugivorous bat Cy. brachyotis shares the same clade with Malaysian isolate (in clade 2). The percentage of trees in which the associated taxa clustered together is shown next to the branches. BS values greater than 50% are shown in the figure. The other clades, consisting of Nycteria, Polychromophilus, Plasmodium, and outgroup are collapsed. (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 2 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 2. Images of bats with Hepatocystis positive infection based on either microscopic examination or cytb gene PCR amplification and sequencing results: H. larvatus (a), H. bicolor (b), H. armiger (c), H. lekakuli (d), R. malayanus (e), R. thomasi (f), R. pearsonii (g), C. thonglongyai (h), and Cy. brachyotis (i). Giemsa-stained blood smears depicting young gametocytes of Hepatocystis in ring and amoeboid forms (j–l), growing and fully-grown macrogametocytes (female) (m–o), growing and fully-grown microgametocytes (male) (p–r) observed in H. larvatus (sample ID THBat19-037, cytb accession no. MT136132). All parasite images were taken at the same magnification. Scale bar = 5 μm. (For viewing the images in color, the reader is referred to the online version of this article). (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 3 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 3. Images of bats with Nycteria positive infection based on either microscopic examination or cytb gene PCR amplification and sequencing results: M. spasma (a), C. thonglongyai (b), T. melanopogon (c), and E. spelaea (d). Giemsa-stained blood smears depicting very early gametocyte (e) with chromatin dot pointed by arrowhead, young and growing macrogametocytes (female) (f–g), growing and fully-grown macrogametocytes (h–k), and growing and fullygrown microgametocytes (l–m) of Nycteria observed in M. spasma (sample ID THBat19- 177, cytb accession no. MT136163). All parasite images were taken at the same magnification. Scale bar = 5 μm. (For viewing the images in color, the reader is referred to the online version of this article). (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 1 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 1. Map of Thailand depicting the bat sampling sites, forested areas, and altitudes. The map was drawn using ArcGIS version 10.2. Altitudes (in meter scale) are indicated in parentheses after each sampling site and were calculated by DIVA-GIS version 7.5.0.0 using spatial data from SRTM DEM Digital Elevation Database.
Fig. 4 in First molecular investigation of haemosporidian parasites in Thai bat species
Fig. 4. Images of bats with Polychromophilus positive infection based on either microscopic examination or cytb gene PCR amplification and sequencing results: My. siligorensis (a) and T. melanopogon (b). Giemsa-stained blood smears depicting growing and fully-grown macrogametocytes of Polychromophilus murinus observed in My. siligorensis (c–e) (sample ID THBat19-211, cytb accession no. MT136168). Growing and fully-grown macrogametocytes of Polychromophilus melanipherus observed in T. melanopogon (f–h) (sample ID THBat19- 170, cytb accession no. MT136167). Fullygrown microgametocytes of P. murinus (i–k). All parasite images were taken at the same magnification. Scale bar = 5 μm. (For viewing the images in color, the reader is referred to the online version of this article). (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)
Fig. 2 in Neglected parasite reservoirs in wetlands: Prevalence and diversity of avian haemosporidians in waterbird communities in Northeast China
Fig. 2. Diversity (a) and frequency (b) of haemosporidian parasite lineages obtained from waterbirds in Tumuji, China. Sankey diagrams of the correlation between waterbirds (left, sorted by order) and identified haemosporidian lineages (right). The width of the lines indicates proportion to the infection recordings in waterbirds, and the colour of the lines indicates the range of the lineage size. The numbers represent infection cases. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)
Fig. 3 in Neglected parasite reservoirs in wetlands: Prevalence and diversity of avian haemosporidians in waterbird communities in Northeast China
Fig. 3. Bayesian phylogenetic reconstruction of 479 bp haemosporidian cyt b lineages from waterbirds in Tumuji, China, with Hepatocystis sp. as an outgroup, and several morpho-species were included for a higher resolution of phylogenetic patterns. Posterior probabilities higher than 0.90 are shown by the node. Lineages that were previously recorded and detected in this study are marked in bold. Major monophyletic clades with high support are labelled behind the line (Leucocytozoon: L1-L5; Haemoproteus: H1–H3).
Fig. 1 in Neglected parasite reservoirs in wetlands: Prevalence and diversity of avian haemosporidians in waterbird communities in Northeast China
Fig. 1. Heatmap of the apparent prevalence of waterbird species in the Tumuji National Nature Reserve. Presenting infected waterbird species (left, sorted by order) with prevalence (indicated by colour gradient, scale from 0 to 1). The sample size is shown in parentheses.
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