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Fig. 2 in Blood recovery of wild Mekong snail-eating turtles (Malayemys subtrijuga Schlegel and Müller, 1845) in captivity from leech infestation
Fig. 2. Analysis of the mean weight of Malayemys subtrijuga during captivity recovery from 2 November 2018 (week 0) to 1 March 2019 (week 17).
Fig. 4 in First report of a severe nasopulmonary acariasis caused by Orthohalarachne diminuata Doetschman, 1944 (Acari: Halarachnidae) in a captive South American sea lion (Otaria flavescens Shaw, 1800)
Fig. 4. ML tree based on 16S rDNA sequences. I. ricinus and D. reticulatus were used as outgroups. Bootstrap values of>70% are shown.
Fig. 3 in First report of a severe nasopulmonary acariasis caused by Orthohalarachne diminuata Doetschman, 1944 (Acari: Halarachnidae) in a captive South American sea lion (Otaria flavescens Shaw, 1800)
Fig. 3. Retrospective evaluation of ante mortem examinations. (A) Dorsal and (B) cranial view of computed tomography (CT) of lung field, revealing marginal emphysematous bullae potentially associated with O. diminuata infestations (arrows). (C) Macroscopically visible mite and mucous in bronchoalveolar lavage (BAL) fluid.
Fig. 2 in First report of a severe nasopulmonary acariasis caused by Orthohalarachne diminuata Doetschman, 1944 (Acari: Halarachnidae) in a captive South American sea lion (Otaria flavescens Shaw, 1800)
Fig. 2. Morphological identification of Orthohalarachne diminuata. Light microscopy of (A) hexapod larval stage and (B) adult female. (C, D, E) Scanning electron microscope (SEM) images of (C) a larval stage, revealing (D) the anterior end of a pedipalp and (E) claw of first leg, showing hair-like sensillae. Scale bars: (A, B, C) 200 μm, (D) 10 μm, (E) 20 μm.
Fig. 1 in First report of a severe nasopulmonary acariasis caused by Orthohalarachne diminuata Doetschman, 1944 (Acari: Halarachnidae) in a captive South American sea lion (Otaria flavescens Shaw, 1800)
Fig. 1. Severe Orthohalarachne diminuata infestation in a 2-year-old South American sea lion. (A) Bifurcatio tracheae reveals various adult mites migrating out of bronchial system. (B) Hyperemic tracheal vessels and adult mites. (C) Trepanation of nasal cavity and sinus paranasalis. (D, E) Multiple clusters of larval mites infesting turbinate mucosa. (F, G) Larval mites burying their pedipalpes and legs into the turbinate mucosa and causing multiple petechial hemorrhages and hyperemia of mucosa. (H) Histological cross-section of turbinate mucosa, showing larval mite (ha), surrounded by saniserous exsudate (hb), and epithelial exfoliation (hc). Legend: White arrows = O. diminuata. Scale bars: (F, G) 2 mm, (H) 200 μm.
Fig. 4 in Giardia duodenalis in a clinically healthy population of captive zoo chimpanzees: Rapid antigen testing, diagnostic real-time PCR and faecal microbiota profiling
Fig. 4. | Faecal bacterial community profile of captive chimpanzees infected with Giardia duodenalis detected by rapid antigen test. (A) Relative abundance of colour coded bacterial phyla separated based on presence (+) or absence (‒) of Giardia using rapid antigen test (RAT). The sample identity is located at the bottom of the graph with two labels (C20, C3) shaded indicating samples that were found as Giardia positive by real-time PCR. (B) Alpha diversity based on observed OTU and Shannon's index plotted as box plot and evaluated using t-tests. (C) Principal coordinates analysis (PCoA) 2D plot using first two principal components from Bray-Curtis dissimilarity matrix at the genus taxonomic levels. The clustering between Giardia positive (RAT+) and negative (RAT-) samples was tested using ANOSIM. (D) Linear discriminant analysis effect size (LEfSe) used plot of significant factors discriminating G. duodenalis positive from negative sample. (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 Giardia duodenalis in a clinically healthy population of captive zoo chimpanzees: Rapid antigen testing, diagnostic real-time PCR and faecal microbiota profiling
Fig. 3. | Faecal bacterial community profile of captive chimpanzees infected with Giardia duodenalis as detected by rapid antigen test and real-time PCR combined. (A) Relative abundance of colour coded bacterial phyla separated based on presence (+) or absence (‒) of Giardia. The sample identity is located at the bottom of the graph. (B) Alpha diversity based on observed OTU and Shannon's index plotted as box plot and evaluated using t-tests. (C) Principal coordinates analysis (PCoA) 2D plot using first two principal components from Bray-Curtis dissimilarity matrix at the genus taxonomic levels. The clustering between Giardia positive (+) and negative (‒) samples was tested using ANOSIM. (D) Linear discriminant analysis effect size (LEfSe) used plot of significant factors discriminating G. duodenalis positive from negative sample. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)
Fig. 2 in Giardia duodenalis in a clinically healthy population of captive zoo chimpanzees: Rapid antigen testing, diagnostic real-time PCR and faecal microbiota profiling
Fig. 2. | Results of Giardia duodenalis rapid antigen test applied on faecal samples from chimpanzees. A positive result for the Giardia duodenalis rapid antigen test (RAT, Anigen Rapid Giardia AG Test Kit) is represented by the line in the 'T' position in the window along with the positive control line in the 'C' position.
Fig. 1 in Giardia duodenalis in a clinically healthy population of captive zoo chimpanzees: Rapid antigen testing, diagnostic real-time PCR and faecal microbiota profiling
Fig. 1. Captive chimpanzees and their enclosure in Sydney, Australia. (A) Main chimpanzee open air exhibit with multiple climbing structures. (B) View from the other direction showing entry to the indoor area at the end of the exhibit. (C) smaller exhibit with mesh covering and more climbing and sleeping structures. (D) Members of the chimpanzee troop at the Taronga Zoo.
Fig. 2. Maximum likelihood tree constructed from partial cox1 in Spirometra infection in a captive Samar cobra (Naja samarensis) in the United States: An imported case?
Fig. 2. Maximum likelihood tree constructed from partial cox1 gene sequences of Spirometra samples and related taxa. HKY + G + I was used as the best substitution model. Schistocephalus solidus and Dibothriocephalus nihonkaiensis were used as outgroups. (JPN – Japan; KOR – South Korea; CHI and CHN – China; AUS – Australia; IRA – Iran; USA – United States; THA – Thailand; MMR – Myanmar; TZA – Tanzania; IND – India; VNM – Vietnam; KHM – Cambodia; LAO – Laos; COL – Colombia; NZL – New Zealand; IDN – Indonesia; ROU – Romania; SSD – South Sudan; ETH – Ethiopia; POL – Poland; UKR – Ukraine; FIN – Finland; CHL – Chile; BRA – Brazil).
Fig. 1. A in Spirometra infection in a captive Samar cobra (Naja samarensis) in the United States: An imported case?
Fig. 1. A) Presence of Spirometra plerocercoid in subcutaneous tissue of a male Samar cobra (Naja samarensis) from a zoological facility in the USA; B) Plerocercoids isolated from de subcutaneous tissue of the same specimen.
Figure 5 in Husbandry, captive breeding, larval development and stages of the Malayan horned frog Megophrys nasuta (Schlegel, 1858) (Amphibia: Anura: Megophryidae)
Figure 5. Megophrys nasuta larvae in stages 18 to 22; blue color is caused by the blue cellular material at the aquarium ground / background while taking photographs. Photos: R. Bach, T. Ziegler, D. Karbe.
Figure 2 in Husbandry, captive breeding, larval development and stages of the Malayan horned frog Megophrys nasuta (Schlegel, 1858) (Amphibia: Anura: Megophryidae)
Figure 2. Megophrys nasuta at the amphibian breeding unit at the Cologne Zoo a) calling male, b) couple in ampleXus during egg deposition, c) embryos, and d) hatched larvae with yolk sacs. Photos: D. Karbe, A. Heidrich, T. Ziegler.
Figure 1 in Husbandry, captive breeding, larval development and stages of the Malayan horned frog Megophrys nasuta (Schlegel, 1858) (Amphibia: Anura: Megophryidae)
Figure 1. Megophrys nasuta enclosures in the amphibian breeding unit at the Cologne Zoo: a) terrarium of the adults, b) rearing tank for larvae at early developmental stages, c) aquaria for advanced larval stages, and d) rearing terraria for juveniles. Photos: D. Karbe.
Figure 4 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 4. Seven species of frogs were included in a husbandry research and technician training program during the first year of the project. The IUCN Red List status, in parenthesis, follows species. A) Heterixalus betsileo (LC). B) Mantidactylus betsileanus, (LC). C) Heterixalus punctatus (LC). D) Blommersia blommersae (LC). E) Guibemantis aff. albolineatus "Andasibe" (DD). F) Stumpffia sp. "Ranomafana" (DD). G) Boophis pyrrhus (LC).
Figure 3 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 3. Terraria and aquaria at the breeding facility. A) Terraria setup on shelving and plumbed so wastewater flows into a drain in the floor. B) A terrarium housing a group of Boophis pyrrhus. C) Aquaria for raising tadpoles. D) Boophis pyrrhus tadpoles produced at the facility.
Figure 9 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 9. Pilot study and training exercise on the optimal larval diet for Mantidactylus betsileanus.
Figure 1. The facility was constructed between November 2010 and March 2011 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 1. The facility was constructed between November 2010 and March 2011 from the foundations of an old abandoned forest station. A) Original abandoned building in January 2009. B) Facility construction November 2010. C) Facility construction December 2010. D) Facility construction January 2011.
Figure 8 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 8. Locally-sourced crickets from Andasibe being bred at Mitsinjo's facility. A) Field cricket (Modicogryllus sp.). B) Large field cricket (Modicogryllus sp.). C) Large black cricket (Gryllus sp.). D) Tropical house cricket (Gryllodes sigillatus). E) Cave cricket (Rhaphidophoridae). F) Shelves with boxes housing field crickets and tropical house crickets.
Figure 2 in Building capacity to implement conservation breeding programs for frogs in Madagascar: Results from year one of Mitsinjo's amphibian husbandry research and captive breeding facility
Figure 2. Overview of the biosecure Mitsinjo amphibian captive breeding and husbandry research center as of April 2012.
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Allen Brain Atlas
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Annotated Behaviour and Observability Dataset (ABODe)
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DANDI Archive for NWB datasets
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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.