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opencc-by-4.0Dec 2020View details →

Рис. 1. Карта-схема заказника «УΑыΛь» с местами сбора кровососущих комаров (Diptera, Culicidae). Описание биотопов Αано в тексте. Черной Λинией выΑеΛена схемати- ческая граница заказника Fig. 1. Map of the Nature Reserve "Udyl" with places where blood-sucking mosquitoes were collected (Diptera, Culicidae). Description of biotopes is given in the paper. The black line marks the schematic boundary of the Nature Reserve in Mosquitoes (Diptera, Culicidae) Of The Nature Reserve "Udyl" (Khabarovsk Krai, Russia)

Рис. 1. Карта-схема заказника «УΑыΛь» с местами сбора кровососущих комаров (Diptera, Culicidae). Описание биотопов Αано в тексте. Черной Λинией выΑеΛена схемати- ческая граница заказника Fig. 1. Map of the Nature Reserve "Udyl" with places where blood-sucking mosquitoes were collected (Diptera, Culicidae). Description of biotopes is given in the paper. The black line marks the schematic boundary of the Nature Reserve

opencc-by-4.0Jan 2024View details →

◂Fig. 5 Gametogenesis in male and female Veneriserva pygoclava. A–D Semi-thin histological sections of female Veneriserva pygoclava, stained with toluidine blue. A Cross-section of a female Veneriserva. B Close-up of large mature oocytes without discernible nurse cells. C Developing oocytes attached to mesenteries (mes), and oogonia proliferating from the ventral side of the dorsal blood vessel (bv). D Details of vitellogenic oocytes and nurse cells. Arrowheads indicate brownstained yolk platelets and yolk bodies. E Live sperm cells captured in a light micrograph. F–G Cross-sections of male Veneriserva. Note the absence of a gut in the cross-sections. Abbreviations—ac acicula, acr acrosome, bv blood vessel, coe coelomic cavity, mes mesentery, nc nurse cell, nn nurse cell nucleus, nu sperm cell nucleus, Oo oocyte, on oocyte nucleus, sp spermatogonia, vnc ventral nerve cord in Hardly Venus's servant-morphological adaptations of Veneriserva to an endoparasitic lifestyle and its phylogenetic position within Dorvilleidae (Annelida)

◂Fig. 5 Gametogenesis in male and female Veneriserva pygoclava. A–D Semi-thin histological sections of female Veneriserva pygoclava, stained with toluidine blue. A Cross-section of a female Veneriserva. B Close-up of large mature oocytes without discernible nurse cells. C Developing oocytes attached to mesenteries (mes), and oogonia proliferating from the ventral side of the dorsal blood vessel (bv). D Details of vitellogenic oocytes and nurse cells. Arrowheads indicate brownstained yolk platelets and yolk bodies. E Live sperm cells captured in a light micrograph. F–G Cross-sections of male Veneriserva. Note the absence of a gut in the cross-sections. Abbreviations—ac acicula, acr acrosome, bv blood vessel, coe coelomic cavity, mes mesentery, nc nurse cell, nn nurse cell nucleus, nu sperm cell nucleus, Oo oocyte, on oocyte nucleus, sp spermatogonia, vnc ventral nerve cord

Fig. 3 in Evaluation of blood and muscle tissues for molecular detection and characterization of hematozoa infections in northern pintails (Anas acuta) wintering in California

Fig. 3. Phylogenetic assignment of hematozoa mitochondrial DNA cytochrome b sequences originating from northern pintails collected from the Central Valley of California (asterisks). Reference sequences for Leucocytozoon (white circles), Haemoproteus (grey circles), and Plasmodium (black circles) parasites were obtained from the National Center for Biotechnology Information. Bootstrap support values for differentiation of broad taxonomic groups are indicated. Values reported for Haemoproteus and Plasmodium show support for phylogenetic differentiation from the mixed subclade formed by reference sequences a and b.

Fig. 4. Minimum spanning network for hematozoa mitochondrial DNA cytochrome b in Evaluation of blood and muscle tissues for molecular detection and characterization of hematozoa infections in northern pintails (Anas acuta) wintering in California

Fig. 4. Minimum spanning network for hematozoa mitochondrial DNA cytochrome b haplotypes detected in Central Valley northern pintails. Circles are drawn proportional to the frequency at which haplotypes were observed. Shading represents the sample collection from which haplotypes originated: white (2006– 2007 wing muscle), grey (2011–2012 wing muscle), and black (2011–2012 blood). A single mutation separates nodes unless explicitly indicated by number. Lines separating nodes are drawn to scale unless indicated by a break. Parasite taxa have been abbreviated in haplotype names (Leu = Leucocytozoon, Hae = Haemoproteus and Pla = Plasmodium).

Fig. 1 in Evaluation of blood and muscle tissues for molecular detection and characterization of hematozoa infections in northern pintails (Anas acuta) wintering in California

Fig. 1. Locations in the Central Valley of California from which northern pintail tissue samples were collected. Samples (n in 2006–2007, n in 2011–2012) were collected in the Sacramento Valley sub-region at: (A) Sacramento National Wildlife Refuge (NWR; 44,92), (B) Delevan NWR (35,7), (C) Colusa NWR (0,2), (D) Sutter NWR (0,1), (E) Little Dry Creek State Wildlife Area (SWA; 0,5), (F) Howard Slough SWA (0,1), (G) Yolo SWA (0,8) and (H) a private duck hunting club (0,1). Samples were collected in the San Joaquin Valley sub-region at: (I) San Luis NWR (7,0), (J) Kesterson NWR (4,0), (K) Los Banos SWA (14,0), (L) Volta SWA (10,0), (M) a private duck hunting club (2,0), and (N) Mendota SWA (30,40).

Fig. 2 in Evaluation of blood and muscle tissues for molecular detection and characterization of hematozoa infections in northern pintails (Anas acuta) wintering in California

Fig. 2. Estimated prevalence of Leucocytozoon (white bars), Haemoproteus (grey bars), and Plasmodium (black bars) parasites in northern pintails sampled in the Central Valley of California in 2006–2007 and 2011–2012 using occupancy modeling. Error bars represent 95% confidence intervals around point estimates.

opencc-by-4.0Dec 2015View details →

Fig. 1 in Manifold habitat effects on the prevalence and diversity of avian blood parasites

Fig. 1. Diagram illustrating how conditions of the vector, parasite, host and habitat must all be permissive for pathogen transmission to occur. The outer layer depicts some factors that are currently causing rapid environmental change, which will affect host‾parasite dynamics.

opencc-by-4.0Dec 2016View details →

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.)

opencc-by-4.0Dec 2016View details →

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.

opencc-by-4.0Dec 2016View details →

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).

opencc-by-4.0Aug 2017View details →

Fig. 2 in Temporal and demographic blood parasite dynamics in two free-ranging neotropical primates

Fig. 2. Individual infection status by parasite by year. Strength and thickness of lines are scaled to the number of individuals that took a given infection trajectory from one year to the next. Two diagonal lines span 2012‾2014 because those individuals were not sampled in 2013. The + symbols represent every infection or non-infection found across all individuals in the study.

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Fig. 3 in Temporal and demographic blood parasite dynamics in two free-ranging neotropical primates

Fig. 3. Parasite species richness by species, age class and sex. Colors represent females (black) and males (gray).

opencc-by-4.0Aug 2017View details →

Fig. 1 in Temporal and demographic blood parasite dynamics in two free-ranging neotropical primates

Fig. 1. Annual prevalence of single- and co-infections by species. Prevalence indicated for each parasite (dark gray), and each pairwise combination of parasites (light gray). Numbers near the top of each bar show the exact prevalence; black lines indicate 95% confidence intervals; dots indicate expected levels of co-infection (refer to Section 3.2). M-D is co-occurrence of M. mariae and Dipetalonema spp., D-T is Dipetalonema spp. and T. minasense, and M-T is M. mariae and T. minasense.

Fig. 3 in Molecular insights into the identification and phylogenetics of the cosmopolitan marine fish blood parasite, Haemogregarina bigemina (Adeleorina: Haemogregarinidae)

Fig. 3. Phylogenetic identification of Haemogregarina bigemina from the UK based on 18S rDNA sequences. (a) Maximum parsimony and (b) Maximum likelihood reconstructions revealing the unique position of UK H. bigemina samples outside of the adeleorine groups. For both phylogenies nodal support was calculated using 1000 bootstrap replicates with only values> 50% presented.

Fig. 1 in Molecular insights into the identification and phylogenetics of the cosmopolitan marine fish blood parasite, Haemogregarina bigemina (Adeleorina: Haemogregarinidae)

Fig. 1. Photograph of the fish host Lipophrys pholis, one of the type hosts of Haemogregarina bigemina, screened in this study.

Fig. 2 in Molecular insights into the identification and phylogenetics of the cosmopolitan marine fish blood parasite, Haemogregarina bigemina (Adeleorina: Haemogregarinidae)

Fig. 2. Stages of Haemogregarina bigemina from Giemsa-stained blood films of Lipophrys pholis from the UK. (a) trophozoite, (b) meront, (c–e) dividing meronts, and (f) paired gamonts. Scale bar = 10 μm.

Fig. 5 in Uncovering Trypanosoma spp. diversity of wild mammals by the use of DNA from blood clots

Fig. 5. Map of the distribution of the Trypanosoma spp. identified in this study. Thirteen different trypanosomes species/genotypes/MOTUs were identified, in single and mixed infection, in the blood clot of bats, carnivores and marsupials. The trypanosomes are distributed in five Brazilian biomes (Amazon Forest, Atlantic Forest, Cerrado, Pampa, and Pantanal). Each colored circle indicates different trypanosome species/genotypes/MOTUs. Abbreviations: Brazilian states: AC, Acre; ES, Espírito Santo; GO, Goiás; MS, Mato Grosso do Sul; PB, Paraíba; RJ, Rio de Janeiro; RS, Rio Grande do Sul.

Fig. 3. T in Uncovering Trypanosoma spp. diversity of wild mammals by the use of DNA from blood clots

Fig. 3. T. cruzi clade phylogenetic tree based on 18S (SSU) gene. The tree shows ten different species and genotypes identified in the blood clot of Carnivora, Chiroptera, and Didelphimorphia: T. cruzi (DTUs TcI, TcII and TcIII), T. dionisii, T. rangeli, T. sp. Neobats 2 and 3, T. janseni, and two novel MOTUs (T. sp. DID and T. sp. Neobat 4). The tree was inferred with neighbor-joining. The numbers at the nodes correspond, respectively, to NJ, ML and BI support values for the main branches. The scale-bar shows the number of nucleotide substitutions per site. Trypanosoma lewisi and Trypanosoma microti were used as outgroups.

Fig. 2 in Uncovering Trypanosoma spp. diversity of wild mammals by the use of DNA from blood clots

Fig. 2. Trypanosoma spp. identified in the blood clot of Carnivora, Chiroptera and Didelphimorphia. Each color indicates a different trypanosome species, genotype or mixed infections. (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)

Fig. 4 in Uncovering Trypanosoma spp. diversity of wild mammals by the use of DNA from blood clots

Fig. 4. Lizard/snake/rodent/marsupial clade phylogenetic tree based on 18S (SSU) gene. The tree shows the three different species from the lizard/snake/rodent/ marsupial clade identified in the blood clot of Chiroptera and Didelphimorphia: T. cascavelli, T. gennari, and T. lainsoni. Tree inferred with neighbor-joining. The numbers at the nodes correspond, respectively, to NJ, ML and BI support values for the main branches. The scale-bar shows the number of nucleotide substitutions per site. Trypanosoma serpentis was used as outgroup.