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622 results for “Underwater”
Figure 15 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 15. Phylogeny of the Hydrophiloidea with mapped evolution of tracheal system (A) and mouthparts (B, C). Two alternative ancestral state reconstructions of mouthparts, considering mouthparts of the Pelthydrus-group as: B, piercingsucking; C, chewing (only tribe Laccobiini shown). D, number of species of aquatic genera of Hydrophilidae with known larvae. Colors of branches/bars/pie-charts indicate functional morphology of mouthparts (red = piercing-sucking, blue = chewing, green = filter-feeding) and development of the tracheal system (grey = open; orange = closed).
Figure 12 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 12. Schematic drawing of the piercing-sucking feeding mechanism: 1, sucking channel; 2, epistomal-mandibular coupling system; 3, flexible area.
Figure 13 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 13. Summary of the main structures related with metapneustic respiratory system. A, Tropisternus latus (Brullé, 1837), spiracular chamber, first-instar larva, light microscope photograph, dorsal view. B, Helochares ventricosus Bruch, 1915, spiracular chamber, first-instar larva, light microscope photograph, dorsal view. C, Tropisternus latus (Brullé, 1837), spiracular chamber, first-instar larva, light microscope photograph, dorsal view. D, Helochares ventricosus Bruch, 1915, abdominal spiracle, first-instar larva, light microscope photograph, dorsal view. E–H, Tropisternus setiger Germar, 1824, SEM micrograph: E, spiracular chamber, third-instar larva, ventral view; F, detail of the terminal spiracle with dust filter, third-instar larva, ventral view; G, abdominal spiracle, first-instar larva, dorsal view; H, detail of the closed abdominal spiracles, first-instar larva, dorsal view. I, J, Oocyclus iguazu (Oliva 1996) third-instar larva, SEM micrograph: I, spiracular chamber, dorsal view; J, biforous abdominal spiracle, dorsal view. K, Laccobius kunashiricus Shatrovskiy, 1984, spiracular chamber, third-instar larva, SEM micrograph, dorsal view.
Figure 11 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 11. Summary of the main structures related with piercing-sucking feeding mechanism, SEM micrograph. A, B, Berosus sp., third-instar larva: A, lobular-mandibular coupling system, dorsal view; B, detail of lobular-mandibular coupling system, ventral view. C, Laccobius (Microlaccobius) sp., third-instar larva, left epistomal lobe, dorsal view.
Figure 10 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 10. Frame sequences of videos showing feeding behavior. A, Tropisternus latus Brullé, 1837, note that the larvae raise the head out of water while feeding. B, Hydrophilus (Dibolocelus) palpalis Brullé, 1837. C, Hemiosus dejeanii (Solier, 1849). D, Oocyclus magnifica Hebauer & Wang, 1998. See also Supporting Information, Videos S1–S4.
Figure 5 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 5. Labroclypeal region of larvae with chewing feeding system, SEM micrograph, dorsal view. A, Tropisternus acaragua Bachmann, 1969, first-instar larva. B, Hydrochara caraboides (Linnaeus, 1758), first-instar larva. C, Hydrophilus (Dibolocelus) palpalis Brullé, 1837, second-instar larva. D, Derallus paranensis Oliva, 1981, first instar larva. E, Helochares ventricosus Bruch, 1915, first-instar larva. F, Hydroglobus puncticolle Bruch, 1915, third-instar larva. G, Dactylosternum cacti (LeConte, 1855), third-instar larva. H, Cercyon quisquilius (Linnaeus, 1761), third-instar larva, white arrow indicates labroclypeal notch. Colours: light blue, frontoclypeal region; green, gFR1, group of sensilla of nasale; violet, gFR2, group of sensilla of epistomal lobe.
Figure 1 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 1. Head capsule of larvae with chewing (A–C) and piercing-sucking (D–I) feeding system, SEM micrograph, dorsal view. A, Hydrophilus (Dibolocelus) palpalis Brullé, 1837, second-instar larva. B, Tropisternus setiger Germar, 1824, firstinstar larva. C, Derallus paranensis Oliva, 1981, first instar larva. D, Berosus sp., third-instar larva. E, Hemiosus bruchi Knisch, 1924, third-instar larva. F, Oocyclus iguazu (Oliva 1996), third-instar larva. G, Laccobius kunashiricus Shatrovskiy, 1984, third-instar larva. H, Hybogralius hartmeyeri (Régimbart, 1908), third-instar larva, light microscope photograph. I, Epimetopus mendeli Fikáček et al. 2011, first-instar larva.
Figure 6 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 6. Labroclypeal region of Hemiosus larvae. A, B, Hemiosus bruchi Knisch, 1924, third-instar larva, SEM micrograph, dorsal view: A, labroclypeus; B, left epistomal lobe. C–E, Hemiosus multimaculatus (Jensen-Haarup, 1910), third-instar larva, dorsal view: C, left epistomal lobe, SEM micrograph; D, detail of gFR2 serrated setae, SEM micrograph; E, left epistomal lobe, light microscope photograph. Abbreviations: EpLb, epistomal lobe; NS, nasale. Colours: light blue, frontoclypeal region; green, gFR1, group of sensilla of nasale; violet, gFR2, group of sensilla of epistomal lobe.
Figure 9 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 9. Labium of larvae with chewing (A–B) and piercing-sucking (C–D) feeding system, dorsal view. A, Enochrus sp., first-instar larva, SEM micrograph. B, Derallus sp., first-instar larva, SEM micrograph. C, Berosus sp., third-instar larva, SEM micrograph. D, Oocyclus sapphirus Short & García, 2010, first-instar larva, light microscope photograph.
Figure 3. Piercing-sucking mandibles. A–C in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 3. Piercing-sucking mandibles. A–C, Berosus patruelis Berg, 1885, first-instar larva, SEM micrograph: A, left mandible, ventral view; B, detail of mandibular teeth, ventral view; C, right mandible, dorsal view. D–F, Laccobius hammondi Gentili, 1984, third-instar larva, SEM micrograph, dorsal view: D, left mandible; E, detail of mandibular teeth; F, right mandible. G–I, Oocyclus iguazu (Oliva, 1996) third-instar larva, SEM micrograph, dorsal view; G, left mandible; H, detail of mandibular teeth; I, right mandible.
Figure 4. Piercing-sucking mandibles. A–C in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 4. Piercing-sucking mandibles. A–C, Hybogralius hartmeyeri (Régimbart, 1908), third-instar larva, light microscope photographs, dorsal view: A, left mandible; B, detail of mandibular teeth; C, right mandible. D–F, Epimetopus mendeli Fikáček et al. 2011, first-instar larva, SEM micrograph, dorsal view: D, left mandible; E, detail of mandibular teeth; F, right mandible. Abbreviations: rc1, first retinaculum; rc2, second retinaculum; rc3, third retinaculum; pt, prostheca.
Figure 2 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 2. Chewing mandibles, SEM micrograph, dorsal view. A, Derallus sp., first-instar larva. B, Enochrus sp., firstinstar larva. C, Tropisternus sp., second-instar larva. D, Hydrophilus (Dibolocelus) palpalis Brullé, 1837, first-instar larva. E, Dactylosternum cacti (LeConte, 1855), third-instar larva. F, Cercyon quisquilius (Linnaeus, 1761), third-instar larva. Abbreviations: rc1, first retinaculum; rc2, second retinaculum; rc3, third retinaculum.
Figure 7 in REVIEW Going underwater: multiple origins and functional morphology of piercing-sucking feeding and tracheal system adaptations in water scavenger beetle larvae (Coleoptera: Hydrophiloidea)
Figure 7. Labroclypeal region of Laccobius larvae. A, B, Laccobius kunashiricus Shatrovskiy, 1984, third-instar larva, SEM micrograph, dorsal view: A, labroclypeus; B, left epistomal lobe. C–E, Laccobius (Microlaccobius) sp., third-instar larva, SEM micrograph, dorsal view: C, left epistomal lobe; D; detail of gFR2 setae; E, seta-like cuticular projections of the latero-ventral membranous lobe. Abbreviations: EpLb, epistomal lobe; NS, nasale. Colours: light blue, frontoclypeal region; green, gFR1, group of sensilla of nasale; violet, gFR2, group of sensilla of epistomal lobe.
Fig. 1. A in Underwater Pupation by the Comal Springs Riffle Beetle, Heterelmis Comalensis Bosse, Tuff, and Brown, 1988 (Coleoptera: Elmidae), with an Update on Culture Techniques
Fig. 1. A) Culture container used for Heterelmis comalensis, B) H. comalensis pupa inside a plastic flow-through chamber. The steel mesh ring was used to forcefully keep pupae underwater.
Improving the reliability of underwater gait analysis using wearable pressure and inertial sensors
<p><strong>Improving the reliability of underwater gait analysis using wearable pressure and inertial sensors</strong></p> <p> </p> <p>This work addresses the lack of reliable wearable methods to assess walking gaits in underwater environments by evaluating the lateral hydrodynamic pressure exerted on lower limbs. Sixteen healthy adults were outfitted with waterproof wearable inertial and pressure sensors. Gait analysis was conducted on land in a motion analysis laboratory using an optoelectronic system as reference, and subsequently underwater in a rehabilitation swimming pool. Differences between the normalized land and underwater gaits were evaluated using temporal gait parameters, knee joint angles and the total water pressure on the lower limbs. The proposed method was validated against the optoelectronic system on land; gait events were identified with low bias (0.01s) using Bland-Altman plots for the stride time, and an acceptable error was observed when estimating the knee angle (10.96° RMSE, Bland-Altman bias -2.94°). The kinematic differences between the land and underwater environments were quantified, where it was observed that the temporal parameters increased by more than a factor of two underwater (p<0.001). The subdivision of swing and stance phases remained consistent between land and water trials. A higher variability of the knee angle was observed in water (CV = 60.75%) as compared to land (CV = 31.02%). The intra-subject variability of the hydrodynamic pressure on the foot (CVz = 39.65%) was found to be substantially lower than that of the knee angle (CVz = 67.69%). The major finding of this work is that the hydrodynamic pressure on the lower limbs may offer a new and more reliable parameter for underwater motion analysis as it provided a reduced intra-subject variability as compared to conventional gait parameters applied in land-based studies.</p> <p> </p>
Underwater Image/Turbidity Dataset
<p>An underwater image dataset with accompanying turbidity values measured in FNU.</p>
Sighting data and tactile events logged from mixed-group underwater interactions
<p>Interactions between mammalian social groups are generally antagonistic as individuals in groups cooperate to defend resources from non-members. Members of the family Delphinidae inhabit a three-dimensional habitat where resource defense is usually impractical. Here, we describe a long-term partial fusion of two communities of Atlantic spotted dolphins (<i>Stenella frontalis</i>). The northern community, studied for 30 years, immigrated 160 km to the range of the southern community, observed for 20 years. Both communities featured fission-fusion grouping patterns, strongest associations between adult males, and frequent affiliative contact between individuals. For the five-year period following the immigration, we found members of all age classes and both sexes in mixed groups, but there was a strong bias toward finding immigrant males in mixed groups. Some association levels between males, and males and females, from different communities were as high as the highest within-community associations. Affiliative contacts indicate that these individuals were forming bonds, likely for future mating opportunities. The mixing of two separate social groups with new bond formation is rare in terrestrial mammal groups. Such mixing between spotted dolphin groups suggests that adaptations to respond aggressively to 'outsiders' is diminished in this species and possibly other ecologically similar dolphins.</p>
Underwater leg gait simulation and testbed
<p>Video 1: Underwater gait simulation (Robot Gait.mp4): multibody simulation for the underwater gait in a quadrupedal robot</p> <p>Video 2: Testbed (Testbed.mp4): Tested gait of a one leg in an underwater environment.</p>
UnderWater Photogrammetry workshop
Source: Objaverse 1.0 / Sketchfab
BVI-Coral: Underwater scenes for 3D reconstruction
<p>The BVI-Coral dataset was captured underwater specifically for 3D reconstruction, with the videos being moved around the target.</p> <p>There are two sets available: the original videos (Originalxxxxx) and the edited versions (HDxxxxx).</p> <p>Please cite our work:</p> <ul> <li>H. Wang, N. Anantrasirichai, F. Zhang and D. Bull, "<a href="https://www.computer.org/csdl/proceedings-article/wacv/2025/108300d287/25Km5swfXQQ">UW-GS: Distractor-Aware 3D Gaussian Splatting for Enhanced Underwater Scene Reconstruction</a>," <em>IEEE/CVF Winter Conference on Applications of Computer Vision (WACV)</em>, 2025.</li> <li>L. Gough, A. Azzarelli, F. Zhang, N. Anantrasirichai, "<a href="https://arxiv.org/html/2502.16351v1">AquaNeRF: Neural Radiance Fields in Underwater Media with Distractor Removal,</a>" <em>IEEE International Symposium on Circuits and Systems, </em>2025.</li> </ul>
ScienceDex guides
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These curated guides explain access requirements, typical timelines, costs, and reuse considerations for widely used research datasets.
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.