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Crustacean Zooplankton Species Richness in 66 North American Lakes
Data from 66 North American lakes were collected to construct a model for predicting the number of crustacean zooplankton species expected in a lake. The chosen lakes have a range from 4 sq m to 80 x 10**9 sq m surface area, range from ultra-oligotrophic to hypereutrophic, and have zooplankton species lists based of several years of observation The number of crustacean zooplankton species in a lake is significantly correlated with lake size, average rate of photosynthesis (parabolic function) and the number of lakes within 20 km. A multiple linear regression model, using these three independent variables, explains approximately 75% of the variation in log species richness. Prediction of species richness is not enhanced by the knowledge of lake depth, salinity, elevation, latitude, longitude, or distance to nearest lake. The North American species area curve is statistically different from and steeper than the corresponding European curve. Number of sites: 69
Crustacean and rotifer density and biomass for Beaverdam Reservoir, Falling Creek Reservoir, Carvins Cove Reservoir, Gatewood Reservoir, and Spring Hollow Reservoir in southwestern Virginia, USA 2014-2025
Crustacean and rotifer density and biomass were measured from 2014 to 2025 in five drinking water reservoirs in southwestern Virginia, USA. These reservoirs are: Beaverdam Reservoir (Vinton, Virginia), Falling Creek Reservoir (Vinton, Virginia), Carvins Cove Reservoir (Roanoke, Virginia), Gatewood Reservoir (Pulaski, Virginia), and Spring Hollow Reservoir (Salem, Virginia). Beaverdam, Falling Creek, Carvins Cove, and Spring Hollow Reservoirs are owned and operated by the Western Virginia Water Authority as primary or secondary drinking water sources for Roanoke, Virginia, and Gatewood Reservoir is a drinking water source for the Town of Pulaski, Virginia. The dataset consists of integrated vertical tow samples from the whole water column, just the epilimnion, and just the hypolimnion (as the difference between the full water column and epilimnion tows), as well as discrete depth measurements collected with a Schindler trap. Most samples were collected at the deepest site of each reservoir adjacent to the dam. Sampling frequency and duration varied among reservoirs and years and included weekly to monthly routine monitoring as well as intensive 24-hour sampling campaigns. In 2014-2016, zooplankton samples were collected approximately fortnightly in the spring, summer, and autumn months at Beaverdam Reservoir, Carvins Cove Reservoir, and Gatewood Reservoirs. Falling Creek Reservoir samples were collected weekly to monthly in spring and summer 2014, and Spring Hollow Reservoir samples were collected approximately fortnightly in the spring, summer, and autumn months of 2015 and 2016. In 2019, zooplankton samples were collected approximately weekly to monthly from April to November at Beaverdam Reservoir and April to September at Falling Creek Reservoir. In 2020, zooplankton samples were collected approximately weekly to monthly from May to December at Beaverdam Reservoir and June to September at Falling Creek Reservoir. In 2021, zooplankton were collected monthly from M
Interagency Ecological Program: San Francisco Bay Study Survey for Fish and Mobile Crustaceans 1980-2024
The San Francisco Bay Study (Bay Study) was established in 1980 to determine the effects of freshwater outflow on the abundance and distribution of fish and mobile crustaceans (brachyuran crabs and caridean shrimp) in the San Francisco Estuary, mainly downstream of the Sacramento-San Joaquin Delta. The Bay Study survey currently samples 52 open-water stations monthly from a research vessel with two types of trawl gear: a midwater trawl to sample pelagic fishes, and an otter trawl to sample demersal fishes, crabs, and shrimp. Historically, the study also included plankton sampling (1980-1989) for larval fish and crustaceans. Fish collected by the otter and midwater trawl are identified to species, counted, and a representative subsample is measured. In addition, crabs from the otter trawl are identified, counted, sexed, and measured, and gelatinous zooplankton from the midwater trawl are identified and counted. Shrimp are retained from each otter trawl sample and returned to the laboratory for processing, which includes identification, counts, sex, and length. Additional data collected at each station includes water depth, Secchi, and a water column profile of temperature and conductivity. This data publication includes fish, crab, shrimp, gelatinous zooplankton (jellies), and water quality data. Metadata related to the plankton sampling will be included in the future when this data is published.
Long-term live imaging, cell identification and cell tracking in regenerating crustacean legs
<p>Supplementary data and videos for the manuscript 'Long-term live imaging, cell identification and cell tracking in regenerating crustacean legs', by Çevrim,<sup> </sup>Laplace-Builhé,<sup> </sup>Sugawara, Rusciano, Labert, Brocard, Almazán and Averof.</p> <p>The supplementary data include:</p> <p><strong>Supplementary Data 1 (.csv file); Live imaging of regenerating <em>Parhyale</em> legs: image acquisition settings</strong></p> <p>Table with information on the 22 time lapse recordings presented in Figure 3, including image acquisition settings, temperature and duration of the recordings.</p> <p><strong>Supplementary Data 2 (.zip file); Live imaging of regenerated <em>Parhyale</em> legs: maximum projections</strong></p> <p>Compressed folder including maximum projections for each of the 22 time lapse recordings presented in Figure 3. These files were generated by projecting all or a subset of the z slices acquired at each time point. A 20 micron scale bar was added on the first time point. These files serve as a quick way to examine the 22 time lapse recordings.</p> <p><strong>Supplementary Data 3 (22 .tif files); Live imaging of regenerated <em>Parhyale</em> legs: complete datasets</strong></p> <p>Complete image 3D+T hyperstacks for each of the 22 time lapse recordings presented in Figure 3. These files have been generated by concatenating the original image stacks and correcting any image shifts, as described in the Methods section of the paper.</p> <p><strong>Supplementary Data 4 (.zip file); Analysis of trade-offs of imaging resolution and image quality</strong></p> <p>The data used for the analysis of trade-offs in imaging and the results shown in Table 1 are included in this compressed folder. Folders for the original recording (labelled 00), for each of the subsampled datasets (labelled 01 to 05), and for the denoised and deconvoluted datasets each include the corresponding image data and ground truth cell tracking files (.tif, .h5, .xml and .mastodon files) and three sets of cell track predictions (.mastodon files). There are also separate folders containing the Elephant detection and flow model parameters for each set of predictions.</p> <p dir="ltr"><strong>Supplementary Data 4 (.zip file); Analysis of trade-offs of imaging resolution and image quality</strong></p> <p dir="ltr">The data used for the analysis of trade-offs in imaging and the results shown in Table 1 are included in two folders. The folder named Image_and_tracking_data includes the image data (.tif, .h5, .xml), ground truth cell tracking files (.mastodon files) and three sets of cell track predictions (.mastodon files) for the original recording (labelled 00), for each of the subsampled datasets (labelled 01 to 05), and for the denoised and deconvoluted datasets. It also includes separate folders containing the Elephant detection and flow model parameters for each set of predictions. The folder named CTC_tracking_results includes the ground-truth data along with three sets of predictions for detection and tracking for each dataset, following the Cell Tracking Challenge format. For each dataset we include label image files (.tif) for every time point along with tracking results in .txt format, and each results directory (01_RES_*) also contains the evaluation results from the Cell Tracking Challenge Evaluation Software. For a detailed explanation of the folder structure, please refer to the Cell Tracking Challenge documentation.</p> <p><strong>Supplementary Data 5 (.zip file); Tracking the progenitors of spineless-expressing cells in the distal carpus</strong></p> <p>The data used to generate Figure 7 are included in this compressed folder, including the live imaging and cell tracking files (.h5, .xml and .mastodon files) and the image stack of the spineless and futsch HCR and DAPI stainings (.tif file). Channel 2 shows spineless expression (mostly nascent transcripts in nuclei), as well as background signal in epidermal nuclei (possibly due to photoconversion of DAPI, see Karg & Golic 2018, Chromosoma 127: 235-245) and strong autofluorescence in granular cells (also visible in channel 1, depicting futsch HCR).</p> <p><strong>Supplementary Data 6 (.txt file); Sequences of <em>Parhyale</em> genes targeted by the HCR probes</strong></p> <p>The sequences are provided in FASTA format.</p> <p dir="ltr"><strong>Supplementary Data 7 (.zip file); Apoptosis in legs that have not been subjected to live imaging</strong></p> <p dir="ltr">The data used to generate Figure 2 supplement 2 are contained in this compressed folder, including 9 image stacks of T4 and T5 legs fixed and stained with DAPI 3 days post amputation (with apoptotic nuclei marked) and a .txt file containing the apoptotic cell counts.</p> <p dir="ltr"><strong>Supplementary Data 8 (.zip file); Analysis of tracking performance in relation to imaging depth</strong></p> <p dir="ltr">The data used to generate Figure 5 are contained in this compressed folder, including separate folders for the data extracted from the analysis of datasets #1 to #5. Each folder includes data from three replicates (batches 001 to 003), with .csv files listing the z location of nucleus centroids (in µm) for the nuclei that were incorrectly detected by Elephant – either as false positives (FP) or as false negatives (FN) – and the ground truth data (GT). The folder also includes an .xlsx file gathering all the relevant data and the measurements of precision and recall.</p> <p dir="ltr"><strong>Supplementary Data 9 (.zip file); Detecting the temporal pattern of cell divisions in regenerating legs</strong></p> <p dir="ltr">The data used to generate Figure 4 are contained in this compressed folder, including the five image datasets (.tif, .h5, .xml), the detected cell divisions (.mastodon files), and an .xlxs file containing all the cell divisions counts and graphs.</p> <p><strong>Video 1. Time lapse recording of regeneration in a Parhyale T5 leg (dataset li48-t5)</strong></p> <p>Live imaging of nuclei labelled with H2B-mREFruby (maximum projection of z slices 3-10). Proximal parts of the leg are to the left and the amputation site is at the right of the frame. For annotations of different features please refer to Figure 2. Shortly after leg amputation (0 hpa) hemocytes adhere to the wound. By 16 hpa the wound has melanized. Up to ~32 hpa epithelial cells can be seen migrating and accumulating at the wound, below the melanized scab (Figure 2A,B). Around 31 hpa, the leg tissues become detached from the scab (Figure 2C). At 43 hpa, the carpus-propodus boundary first becomes visible, and thereafter many cells can be observed dividing at the distal part of the leg stump (Figure 2D). At 56 hpa, the propodus-dactylus boundary first becomes visible (Figure 2E). At later stages, tissues in more proximal parts of the leg retract, making space for the regenerating leg to grow (Figure 2F,G). After ~90 hpa cell proliferation there is less cell proliferation and cell movements, and the nuclear positions within the tissue become fixed. Scale bars, 20 µm.</p> <p><strong>Video 2. Time lapse recording of regeneration in a Parhyale T5 leg (dataset li36-t5)</strong></p> <p>Live imaging of nuclei labelled with H2B-mREFruby (maximum projection of z slices 3-15). Proximal parts of the leg are to the left and the amputation site is at the right of the frame. The sequence of events is similar to that described in Video 1, but the progression is slower: epithelial migration towards the wound is observed up to 40 hpa, tissues detach from the scab at 65 hpa, and the carpus-propodus and propodus-dactylus boundaries first become visible at 78 and 91 hpa. The tissues making up the carpus and propodus can be seen pulsating from 105 to 145 hpa. Scale bars, 20 µm.</p>
Sub-fossil crustacean zooplankton relative abundances from 101 lakes across Canada
<p>This data set contains cladoceran sub-fossil relative abundances for 101 lakes across Canada sampled as part of the NSERC Canadian Lake Pulse Network project. Lakes were sampled once, over three summers (2017-2018-2019). Cores were collected using a gravity corer in the deepest point of each lake and were sectioned on site with a vertical extruder. Each lake was sampled for a “top” sediment sample, represented by the first centimeter of the surface of the sediment core, and a “bottom” sediment sample, corresponding to the 1 cm of sediment located between 3 and 4 cm from the base of the core. Cladoceran extraction and preparation followed the protocol from Korhola and Rautio (2001). Cladocerans were identified using DM 2500 Leica compound inverted microscope under 200X-400X magnification with a minimal count size of 100 individuals. Identification at the species, genus, or species complex level followed Szeroczynska and Sarmaja-Korjonen (2007) and Korosi and Smol (2012a; b).</p> <p>Sites are identified with Lake ID number, followed by “T” for top samples and “B” for bottom samples. Lakes IDs with respective locations (longitude and latitude coordinates) and Continental Basin allocations can be found here: <a href="https://doi.org/10.5281/zenodo.4701262">https://doi.org/10.5281/zenodo.4701262</a></p> <p>References</p> <p>Korhola, A., and M. Rautio. 2001. Cladocera and other branchiopod crustaceans, p. 225–234. <em>In</em> J.P. Smol, H.J.B. Birks, and W.M. Last [eds.], Tracking Environmental Change Using Lake Sediments. Springer.</p> <p>Korosi, J. B., and J. P. Smol. 2012a. An illustrated guide to the identification of cladoceran subfossils from lake sediments in northeastern North America: Part 1-the Daphniidae, Leptodoridae, Bosminidae, Polyphemidae, Holopedidae, Sididae, and Macrothricidae. J. Paleolimnol. <strong>48</strong>: 571–586. doi:10.1007/S10933-012-9632-3</p> <p>Korosi, J. B., and J. P. Smol. 2012b. An illustrated guide to the identification of cladoceran subfossils from lake sediments in northeastern North America: Part 2-the Chydoridae. J. Paleolimnol. <strong>48</strong>: 587–622.</p> <p>Szeroczyfiska, K., and K. Sarmaja-Korjonen. 2007. Atlas of Subfossil Cladocera from Central and Northern Europe, Friends of the Lower Vistula Society, Warsaw, Pol.</p>
FIG. 1 in An appraisal of the Middle-Late Miocene fossil decapod crustaceans of the 'Faluns' (Anjou-Touraine, France)
FIG. 1. — Location map of the outcrops area, and extension of the Falun's Sea during the Middle-Late Miocene (shaded area). Map from Gagnaison et al. 2012.?, limits of the "Faluns sea" probable extension.
FIG. 9 in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 9. — Pie charts showing the relative abundances of the crustacean communities from: A, Sainte-Scolasse-sur-Sarthe (late Callovian, Normandy, France; after Chény et al. 2023); B, Haute-Saône (early Oxfordian, east France; after Charbonnier et al. 2012); and C, Cricqueboeuf (late Oxfordian, Normandy, France; present work).
FIG. 8 in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 8. — Eryma ventrosum (Meyer, 1835) from the late Oxfordian of Cricqueboeuf, Normandy: A-C, subcomplete specimen MPV 2013.1.288.61, right lateral, dorsal, and ventral views; D-F, specimen MPV 2013.1.288.56, cephalic region showing the eyes, dorsal view (D), close-up of stalked-eye (E), close-up of ommatidia network (F); G, specimen MPV 2013.1.288.8, P1 chela, outer view; H, specimen MPV 2013.1.288.39, P1 chela, index and propodus, inner view; I, J, isolated pleon MPV 2013.1.288.50, dorsal and right lateral views; K, specimen MPV 2013.1.288.60, close-up of tail fan. Abbreviations: ip, intercalated plate; o, eye; os, orbital spine; r, rostrum. Photographs: L. Cazes, except (E-F): D. Audo. Scale bars: A-C, G-K, 1 cm; D, 5 mm; E, 1 mm; F, 200 μm.
FIG. 7 in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 7. — Eryma ventrosum (Meyer, 1835) from the late Oxfordian of Cricqueboeuf, Normandy: A, carapace MPV 2013.1.288.2, right lateral view; B, carapace MPV 2013.1.288.13, left lateral view; C, carapace MPV 2013.1.288.54, right lateral view; D, carapace MPV 2013.1.288.28, partially enclosed in carbonate nodule, right lateral view; E-G, carapace MPV 2013.1.288.57, interpretative line drawing, right lateral and ventral views; H, carapace MPV 2013.1.288.49, close-up of cephalic region, note the strong orbital and antennal spines; I, carapace MPV 2013.1.288.8, close-up of antennal-pterygostomial and ventral regions. Abbreviations: a, branchiocardiac groove; as, antennal spine; b, antennal groove; b1, hepatic groove; c, postcervical groove; d, gastro-orbital groove; ep, epistome; e1e, cervical groove; i, inferior groove; md, mandible; os, orbital spine; PoA, postorbital area; r, rostrum. Photographs: L. Cazes. Line drawings: S. Charbonnier. Scale bars: 5 mm.
FIG. 6. — Meyeria hurtrelleorum n in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 6. — Meyeria hurtrelleorum n. sp. from the late Oxfordian of Cricqueboeuf, Normandy: A-C, paratype MPV 2013.1.289.2, carapace and pleon in connection, dorsal and right lateral views, and interpretative line drawing; D, paratype MPV 2013.1.289.2, carapace and close-up of pleonal somites 2 and 3, right lateral view; E, F, paratype MPV 2013.1.289.4, fragment of carapace and P1 merus, left lateral and dorsal views; G, paratype MPV 2013.1.289.4, close-up of carapace, left lateral view; H, subcomplete specimen MPV 2013.1.289.18, almost totally enclosed in carbonate nodule showing yellowish quartz grains and ferrugineous oolites; I, J, specimen MPV 2013.1.289.58 always enclosed in enclosed in carbonate nodule showing large, yellowish quartz grains. Abbreviations: a, branchiocardiac groove; c, postcervical groove; cd, cardiac groove; dm, dorsal midline; e1e, cervical groove; oc, orbital carina; r, rostrum; sc, scaphocerite; s1-s3, pleonal somites 1 to 3. Photographs: L. Cazes. Line drawing: S. Charbonnier. Scale bars: 5 mm.
FIG. 4. — Meyeria hurtrelleorum n in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 4. — Meyeria hurtrelleorum n. sp. from the late Oxfordian of Cricqueboeuf, Normandy: A, holotype MPV 2013.1.289.1, dorsal view; B, C, paratype MPV 2013.1.289.11, carapace and pleon, right lateral view and interpretative line drawing; D, paratype MPV 2013.289.14, subcomplete specimen always enclosed into a carbonate concretion, left lateral view; E, paratype 2013.289.10, subcomplete specimen, left lateral view; F, paratype 2013.289.15, isolated carapace, left lateral view, note the coarse matrix with yellowish quartz grains; G-I, paratype 2013.289.15, carapace and pereiopods, right lateral and dorsal views, and interpretative line drawing, note the well-preserved subchelate pereiopod 2. Abbreviations: a, branchiocardiac groove; ac, antennal carina; b, antennal groove; b1, hepatic groove; c, postcervical groove; cd, cardiac groove; dm, dorsal midline; e1e, cervical groove; gc, gastro-orbital carina; i, inferior groove; oc, orbital carina; r, rostrum; sc, scaphocerite; s1-s5, pleonal somites 1 to 5. Photographs: L. Cazes. Line drawings: S. Charbonnier. Scale bars: 5 mm.
FIG. 5. — Meyeria hurtrelleorum n in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 5. — Meyeria hurtrelleorum n. sp. from the late Oxfordian of Cricqueboeuf, Normandy: A-C, paratype MPV 2013.1.289.5, subcomplete specimen showing carapace, pleon, and fragments of pereiopods, right lateral and left lateral views, and interpretative line drawing of pleon; D, E, paratype MPV 2013.1.289.74, carapace in right lateral and dorsal views; F, paratype MPV 2013.1.289.6, two specimens enclosed into the same nodule, dorsal view, note one large yellowish quartz grain (white arrow); G, paratype MPV 2013.1.289.9, subcomplete specimen, dorsal view; H-I, paratype IGR-PAL-153418, subcomplete specimen, dorsal view (H) and close-up of telson (I); J, paratype MPV 2013.1.289.12, close-up of telson, note epibiotic mollusc bivalve fixed on distal part (white arrow); K, paratype MPV 2013.1.289.16, carapace and pleon, left lateral view. Abbreviations: P1m, merus of first pereiopod; s1-s6, pleonal somites 1 to 6; t, telson. Photographs: L. Cazes, except: I, D. Gendry. Line drawing: S. Charbonnier. Scale bars: 5 mm.
FIG. 1 in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 1. — Geographic and geological settings: A, location of the Cricqueboeuf outcrop in Normandy;B, stratigraphic log of the upper Oxfordian- lower Kimmeridgian succession based on Guyader (1968) and modified after Devillez et al. (2018). The red arrow indicates the interval of beds yielding crustacean-bearing nodules.
FIG. 2 in The decapod crustacean fauna from the Late Jurassic of Cricqueboeuf, Normandy (France)
FIG. 2. — Glypheopsis trouvillensis Charbonnier, Garassino, Schweigert & Simpson, 2013 from the late Oxfordian of Cricqueboeuf, Normandy: A, B, carapace MPV 2023.1.146.5 and interpretative line drawing, left lateral view; C, carapace IGR-PAL-153416, right lateral view; D, carapace MPV 2013.1.146.3, right lateral view; E, carapace MPV 2013.1.146.4, left lateral view; F, carapace MPV 2013.1.146.6, right lateral view; G-I, carapace IGR-PAL-153417, right lateral, left lateral and dorsal views. Abbreviations: a, branchiocardiac groove; ac, antennal carina; b, antennal groove; b1, hepatic groove; c, postcervical groove; cd, cardiac groove; e1e, cervical groove; gc, gastro-orbital carina; i, inferior groove; ic, intercervical groove; oc, orbital carina; Photographs: L. Cazes, except (C): D. Gendry. Line drawing: S. Charbonnier. Scale bars: 5 mm.
Figure 10. Simple setae. A in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 10. Simple setae. A, typical simple setae from the mandibular palp of Panulirus argus. No outgrowths are seen. B, terminal pore (arrow) from simple seta. C, simple setae situated on the basis of maxilla 2 of Carcinus maenas. Abbreviation: Si, simple setae.
Figure 5. Pappose setae. A in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 5. Pappose setae. A, overview of two typical pappose setae from Cherax quadricarinatus. Note random arrangement of setules. B, tips of pappose setae from Stenopus hispidus. Setules get smaller closer to the tip (arrow). C, serration on the setules (arrows) from pappose seta. D, pappose setae on the exopod of maxilliped 1 of Carcinus maenas. E, pappose setae on the mandibular palp of Ca. maenas. F, pappose setae on the coxa of maxilliped 1 of Pagurus bernhardus. Abbreviation: Pa, pappose setae.
Figure 4 in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 4. Substructures of setae. A, infracuticular articulation with the general cuticle. Arrow indicates deep socket. B, supracuticular articulation (arrows) with the general cuticle. C, annulus seen as a ring in the cuticle (arrow). D, two rows of denticles arranged distally on a seta. E, large setule displaying articulation (arrow) with setal shaft. F, small setule with weak articulation (arrows). G, stitched picture showing gradual change from setule (arrow) to denticle (arrowhead) on the same seta. H, subterminal pore (arrow) from seta with denticles. I, terminal pore (arrow) from seta with denticles.
Figure 7. Serrulate setae. A, typical serrulate setae from maxilliped 1 in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 7. Serrulate setae. A, typical serrulate setae from maxilliped 1 of Pagurus bernhardus. Setules are small and only present on the distal half of the seta. B, middle part of serrulate seta with setules in three rows. C, setules from serrulate seta arranged randomly along the shaft. Note strong serration. D, small setules with weak articulations (arrows). E, scalelike setules from serrulate seta of Palaemon adspersus. Note serration on distal rim (arrows). F, terminal pore (arrow) from serrulate seta. G, serrulate setae on the coxa of maxilla 1 of Penaeus monodon. Abbreviation: Su, serrulate setae.
Figure 9. Papposerrate setae. A, typical papposerrate seta from maxilliped 1 in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 9. Papposerrate setae. A, typical papposerrate seta from maxilliped 1 of Cherax quadricarinatus, with long, randomly arranged setules on proximal part and denticles in two rows on distal part. B, transition region between long setules and denticles. Abbreviations: D, denticles; LS, long setules; SS, short setules.
Figure 8. Serrate setae. A in Revising the definition of the crustacean seta and setal classification systems based on examinations of the mouthpart setae of seven species of decapods
Figure 8. Serrate setae. A, typical serrate setae from the endopod of maxilla 1 of Cherax quadricarinatus. Denticles in two strict rows on the distal half. B, serrate seta with setules (arrow). Arrowhead indicates denticles. C, tip of serrate seta with terminal pore (arrow). No denticles, only scale-like setules near the tip (arrowhead). D, partial (arrows) and complete fusion of denticles on serrate seta from Penaeus monodon. E, serrate setae on the dactylus of maxilliped 3 of Palaemon adspersus. F, serrate setae on the dactylus of maxilliped 2 of Pe. monodon. Abbreviation: Se, serrate setae.
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Allen Brain Atlas
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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.
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OpenNeuro
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