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Distribution. The Gedemsa is now restricted to five isolated locations in the Bale and Arsi Mt ranges of SC Ethiopia, S and SE of the Rift Valley. in Bovidae
Distribution. The Gedemsa is now restricted to five isolated locations in the Bale and Arsi Mt ranges of SC Ethiopia, S and SE of the Rift Valley.
Distribution. Discontinuous and limited to wetland environments in the Congo Basin N and W of the range of the Zambezi Sitatunga in S Benin (Porto Novo), S Nigeria, Cameroon, Central African Republic, Equatorial Guinea, Gabon, Republic of the Congo, N DR Congo; also several isolated populations in W Africa (Senegal, Gambia & Guinea-Bissau), NE Nigeria and W Chad, and perhaps extreme S Ghana. Maps and distributional information here are provisional pending future research. in Bovidae
Distribution. Discontinuous and limited to wetland environments in the Congo Basin N and W of the range of the Zambezi Sitatunga in S Benin (Porto Novo), S Nigeria, Cameroon, Central African Republic, Equatorial Guinea, Gabon, Republic of the Congo, N DR Congo; also several isolated populations in W Africa (Senegal, Gambia & Guinea-Bissau), NE Nigeria and W Chad, and perhaps extreme S Ghana. Maps and distributional information here are provisional pending future research.
Distribution. Malayan Tapirs occur in two disjunct and isolated populations, one on mainland SE Asia in peninsular Malaysia, Thailand, and Myanmar, and the other in the S & C Sumatra, in Indonesia. in Tapiridae
Distribution. Malayan Tapirs occur in two disjunct and isolated populations, one on mainland SE Asia in peninsular Malaysia, Thailand, and Myanmar, and the other in the S & C Sumatra, in Indonesia.
Subspecies and Distribution. H.b.bruceiGray,1868—Ethiopia. H.b.albipesHollister,1922—Kenya. H.b.bakeriGray,1874—Uganda. H.b.bocageiGray,1869—Angola. H.b.chapiniHatt,1933—DRCongo. H.b.dieseneriBrauer,1917—Tanzania. H.b.fromm:Brauer,1913—Tanzania. H.b.grantiWroughton,1910—SouthAfrica. H.b.hindeiWroughton,1910—Kenya. H.b.hoogstraaliSetzer,1956—Sudan. H.b.kemp:Thomas,1910—Kenya. H.b.lademanniBrauer,1917—Tanzania. H.b.manningiWroughton,1910—Malawi. H.b.mossambicusPeters,1870—Mozambique. H.b.muenzneriBrauer,1913—Tanzania. H.b.princepsThomas,1910—Ethiopia. H.b.prittwitziBrauer,1917—Tanzania. H.b.pumilusThomas,1910—Somaliland. H.b.rudd:Wroughton,1910—Mozambique. H.b.rudolfiThomas,1910—Ethiopia. H.b.somalicusThomas,1892—Somaliland. H.b.ssongeaeBrauer,1917—Tanzania. H.b.thomasiNeumann,1901—Sudan. H. b. victorianjansae Brauer, 1917 — Tanzania. Endemic to Africa from NE Sudan throughout the Horn of Africa, south to Limpopo and Mpumalanga provinces in South Africa, and also isolated populations in Angola. Determining the limits of subspecific distribution is not possible for the moment, but the subspecies and the countries bearing their type localities are included above. in Procaviidae
Subspecies and Distribution. H.b.bruceiGray,1868—Ethiopia. H.b.albipesHollister,1922—Kenya. H.b.bakeriGray,1874—Uganda. H.b.bocageiGray,1869—Angola. H.b.chapiniHatt,1933—DRCongo. H.b.dieseneriBrauer,1917—Tanzania. H.b.fromm:Brauer,1913—Tanzania. H.b.grantiWroughton,1910—SouthAfrica. H.b.hindeiWroughton,1910—Kenya. H.b.hoogstraaliSetzer,1956—Sudan. H.b.kemp:Thomas,1910—Kenya. H.b.lademanniBrauer,1917—Tanzania. H.b.manningiWroughton,1910—Malawi. H.b.mossambicusPeters,1870—Mozambique. H.b.muenzneriBrauer,1913—Tanzania. H.b.princepsThomas,1910—Ethiopia. H.b.prittwitziBrauer,1917—Tanzania. H.b.pumilusThomas,1910—Somaliland. H.b.rudd:Wroughton,1910—Mozambique. H.b.rudolfiThomas,1910—Ethiopia. H.b.somalicusThomas,1892—Somaliland. H.b.ssongeaeBrauer,1917—Tanzania. H.b.thomasiNeumann,1901—Sudan. H. b. victorianjansae Brauer, 1917 — Tanzania. Endemic to Africa from NE Sudan throughout the Horn of Africa, south to Limpopo and Mpumalanga provinces in South Africa, and also isolated populations in Angola. Determining the limits of subspecific distribution is not possible for the moment, but the subspecies and the countries bearing their type localities are included above.
Subspecies and Distribution. A. g. geoffroyi Kuhl, 1820 — S & SE Nicaragua (coastal region around San Juan del Norte or Martina Bay, probably ranging across the lowlands to the vicinity of Lake Managua and Lake Nicaragua on the Pacific coast); possibly in N Costa Rica. A. g. azuerensis Bole, 1937 — SC Panama, known only from the forested mountains of the W side of the Azuero Peninsula (Veraguas Province) in the vicinity of Ponuga, where it appears to be isolated; it may also occur to the W along the Pacific coastto the Burica Peninsula, near the Panamanian and Costa Rican border. A. g. frontatus Gray, 1842 — N & W Nicaragua and NW Costa Rica. A. g. grisescens Gray, 1866 — S Panama along the Pacific coast in the valley of the Rio Tuyra and SE through the Serrania del Sapo of extreme SE Panama into the Cordillera de Baudo of NW Colombia. A. g. ornatus Gray, 1871 — C & E Costa Rica, and Panama (from Chiriqui Province to the Serrania de San Blas E of the Canal Zone). A. g. vellerosus Gray, 1866 — E & SE Mexico (E San Luis Potosi, Veracruz, Tabasco, E Oaxaca, and Chiapas states), Guatemala (including the highlands), El Salvador, and Honduras (along the N coastto the lowlands of La Mosquitia in Gracias a Dios Department). A. g. yucatanensis Kellogg & Goldman, 1944 — SE Mexico (forests of the Yucatan Peninsula), NE Guatemala, and adjoining parts of Belize; intergrading in S Mexico (Campeche State) and Guatemala with vellerosus. in Atelidae
Subspecies and Distribution. A. g. geoffroyi Kuhl, 1820 — S & SE Nicaragua (coastal region around San Juan del Norte or Martina Bay, probably ranging across the lowlands to the vicinity of Lake Managua and Lake Nicaragua on the Pacific coast); possibly in N Costa Rica. A. g. azuerensis Bole, 1937 — SC Panama, known only from the forested mountains of the W side of the Azuero Peninsula (Veraguas Province) in the vicinity of Ponuga, where it appears to be isolated; it may also occur to the W along the Pacific coastto the Burica Peninsula, near the Panamanian and Costa Rican border. A. g. frontatus Gray, 1842 — N & W Nicaragua and NW Costa Rica. A. g. grisescens Gray, 1866 — S Panama along the Pacific coast in the valley of the Rio Tuyra and SE through the Serrania del Sapo of extreme SE Panama into the Cordillera de Baudo of NW Colombia. A. g. ornatus Gray, 1871 — C & E Costa Rica, and Panama (from Chiriqui Province to the Serrania de San Blas E of the Canal Zone). A. g. vellerosus Gray, 1866 — E & SE Mexico (E San Luis Potosi, Veracruz, Tabasco, E Oaxaca, and Chiapas states), Guatemala (including the highlands), El Salvador, and Honduras (along the N coastto the lowlands of La Mosquitia in Gracias a Dios Department). A. g. yucatanensis Kellogg & Goldman, 1944 — SE Mexico (forests of the Yucatan Peninsula), NE Guatemala, and adjoining parts of Belize; intergrading in S Mexico (Campeche State) and Guatemala with vellerosus.
Subspecies and Distribution. L. c. cana E. Geoffroy Saint-Hilaire, 1812 — Brazilian Amazon, S of the Rio Amazonas-Solimoes, between the rios Jurua and Tapajos-Juruena, but restricted to the left bank of the Rio Madeira above the mouth of the Rio Jiparana (a right bank tributary), and to the right bank of the Rio Jiparana, S to ¢.12° S, and W along the N (left bank) of the Rio Abuna on the upper Rio Madeira. L. c. tschudii Pucheran, 1857 — SE Peru, its range is poorly known butis believed to extend between the rios Pachitea and Ucayali, S from the Rio Inuya, W as far as the Rio Inambari, and S to both sides of the Rio Madre de Dios into the Rio Tambopata Basin, to the frontier with Bolivia, with an isolated population in Madidi National Park. in Atelidae
Subspecies and Distribution. L. c. cana E. Geoffroy Saint-Hilaire, 1812 — Brazilian Amazon, S of the Rio Amazonas-Solimoes, between the rios Jurua and Tapajos-Juruena, but restricted to the left bank of the Rio Madeira above the mouth of the Rio Jiparana (a right bank tributary), and to the right bank of the Rio Jiparana, S to ¢.12° S, and W along the N (left bank) of the Rio Abuna on the upper Rio Madeira. L. c. tschudii Pucheran, 1857 — SE Peru, its range is poorly known butis believed to extend between the rios Pachitea and Ucayali, S from the Rio Inuya, W as far as the Rio Inambari, and S to both sides of the Rio Madre de Dios into the Rio Tambopata Basin, to the frontier with Bolivia, with an isolated population in Madidi National Park.
FIGURE 3. Secondary structures for the D1–D1 in New cyanobacterium Aliterella vladivostokensis sp. nov. (Aliterellaceae, Chroococcidiopsidales), isolated from temperate monsoon climate zone (Vladivostok, Russia)
FIGURE 3. Secondary structures for the D1–D1′ helices in the ITS regions for five Aliterella species and putative genus member Synechocystis sp. PCC 7509. Conservative nucleotides are grey colored.The unique marker mutations for the new species A. vladivostokensis are black colored. Arrowheads show compensatory (CBCs) and hemi-compensatory base changes (hCBCs). Homological base pairs among different species are indicated by dotted lines.
FIGURE 6 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 6 Chlamydospores morphology of wet bubble disease pathogen isolates on diseased basidiomes observed by light microscopy. A–B: Big chlamydospore group. A: Chlamydospore of WH1; B: Chlamydospore of HN0015–8; C–D: Small chlamydospore group. C: Chlamydospore of H1–12; D: Chlamydospore of H3–4. Bar=20 µm.
FIGURE 8 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 8 Chlamydospores morphology of wet bubble disease pathogen isolates on PDA media observed by light microscopy. A–B: Big chlamydosporse group. A: Chlamydospores of WH1; B: Chlamydospores of HN0015–8; C–D: Small chlamydospores group. C: Chlamydospores of H1–12; D: Chlamydospores of H3–4.
FIGURE 10 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 10 The pathogenicity level of WBD pathogen isolates. (A) A healthy basidiome of A. bisporus without inoculation of WBD pathogen isolates, fruiting bodies without brown spots; (B) Highly pathogenicity WBD pathogen isolates, most primordia of A. bisporus differentiated into malformed fruiting bodies; (C) Weak pathogenicity WBD pathogen isolates, most of the primordia of A. bisporus formed normal fruiting bodies, while a part of the fruiting bodies were infected, the pathogen with brown spots and few primordia formed irregular fruiting bodies.
FIGURE 4 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 4 Maximum likelihood tree based on analysis of the ITS, nrLSU and RPB2 sequence data with Trichoderma aureoviride as the outgroup.
FIGURE 5 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 5 Conidiophore and conidia morphology of wet bubble disease pathogen isolates cultured on PDA. A–B: Big chlamydospore group. A: Chlamydospore of WH1, Bar=20 µm; B: Chlamydospore of HN0015–8, Bar=10µm.
FIGURE 9 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 9 Chlamydospores morphology of wet bubble disease pathogen isolates on PDA medium observed by SEM. A–B: Big chlamydospores group. A: Chlamydospore of WH1; B: Chlamydospores of HN0015–8; C–D: Small chlamydospores group. C: Chlamydospores of H1–12; D: Chlamydospores of H3–4.
FIGURE 3 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 3 Maximum likelihood tree based on analysis of the RPB2 sequence data with Trichoderma aureoviride as the outgroup.
FIGURE 7 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 7 Colony morphology of H. perniciosus isolates on PDA media. A: Hypomyces perniciosus WH1 strain colony morphology, colony type (ⅰ); B: Hypomyces perniciosus HN0015–8 colony morphology, colony type (ii); C: Hypomyces perniciosus H1–12 colony morphology, colony type (iii); D: Hypomyces perniciosus H3–4 colony morphology, colony type (iv).
FIGURE 1 in Morphological and phylogenetical analyses of pathogenic Hypomyces perniciosus isolates from Agaricus bisporus causing wet bubble disease in China
FIGURE 1 Maximum likelihood tree based on analysis of the ITS sequence data with Trichoderma aureoviride as the outgroup.
FIGURE 1 in Absidia aguabelensis sp. nov.: A new mucoralean fungi isolated from a semiarid region in Brazil
FIGURE 1. Phylogenetic tree of Absidia aguabelensis URM 8213 and related species based on maximum likelihood (ML) analysis of combined internal transcriber spacer and large subunit of ribosomal DNA. Bootstrap values for Bayesian posterior probabilities over 0.9 and ML greater than or equal to 70% are placed above the branches. Bootstrap values lower than 0.9 and ML less than 70% are marked with "*". The bar indicates the number of substitutions per position. The strain proposed in the current study is shown in bold blue. Cunninghamella phaeospora CBS 692.68 and Cunninghamella vesiculosa CBS 989.96 were used as outgroups.
FIGURE 2 in Absidia aguabelensis sp. nov.: A new mucoralean fungi isolated from a semiarid region in Brazil
FIGURE 2. Absidia aguabelensis sp. nov. (URM 8213). A. Surface of colony on malt extract agar at 25°C. B. Young sporangiophore with sporangium. C. Mature sporangiophores with sporangium, columella, and a bell-shaped apophysis. D, E. Branched sporangiophore; F, G, H, I. Sporangiophore with columella; J. Sporangiospores. Bars: B, C, J = 25 μm; D, E = 50 μm; F, G, H, I = 12.5 μm.
Figure 5 in Geographic isolation and human-assisted dispersal in land snails: a Mediterranean story of Helix borealis and its relatives (Gastropoda: Stylommatophora: Helicidae)
Figure 5. Results of biogeographic reconstruction using the DEC model in RASP using 1000 time-trees estimated with BEAST from the full dataset (see text). Maximum of three areas was allowed for ancestral ranges and unlikely disjunctive ranges were prohibited. The areas (A–F, in parentheses) of which the ranges of the terminals consist are shown in Figure 2.
Figure 2 in Geographic isolation and human-assisted dispersal in land snails: a Mediterranean story of Helix borealis and its relatives (Gastropoda: Stylommatophora: Helicidae)
Figure 2. Distribution of sampling sites and assignment of locally sampled individuals to major mitochondrial clades of the Mediterranean clade of Helix. Different symbols and colours correspond to different groups as in Figure 4. Areas used for biogeographic reconstructions are shown and labelled with letters corresponding to those in Figure 5. A, northern Adriatic basin; B, northern Africa; C, Apennine Peninsula and Corsica; D, Greece, western Aegean and Crete; E, eastern Aegean and western Anatolia; F, northern Levant.
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Allen Brain Atlas
Allen Brain Atlas is an Allen Institute collection of brain map atlases, datasets, APIs, and analysis tools covering mouse, human, and non-human primate brain resources.
Annotated Behaviour and Observability Dataset (ABODe)
ABODe is a University of Edinburgh DataShare dataset for behavior classification in group-housed mice using home-cage video, identities, bounding boxes, ground-plate positions, and annotator labels.
DANDI Archive for NWB datasets
DANDI is a BRAIN Initiative archive for publishing and sharing neurophysiology data, including electrophysiology, optophysiology, and behavioral data packaged as NWB and related standards.
International Brain Laboratory public data
The International Brain Laboratory public data releases expose standardized mouse decision-making experiments, including Neuropixels recordings, widefield calcium imaging, behavior, and session metadata accessed through the ONE API.
OpenNeuro
OpenNeuro is a free, open platform for sharing neuroimaging datasets, with public search, dataset pages, and download paths for web, S3, DataLad, and the OpenNeuro CLI.