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476 results for “morphogenesis”
Plant regeneration in leaf culture of Centaurium erythraea Rafn. Part 3: de novo transcriptome assembly and validation of housekeeping genes for studies of in vitro morphogenesis
<p>Six centaury transcriptomes (embryogenic calli, globular somatic embryos, cotyledonary somatic embryos, adventitious buds, leaves and roots of <em>in vitro</em> grown plants) were sequenced and <em>de novo</em> assembled using <a href="https://github.com/trinityrnaseq/trinityrnaseq/wiki">Trinity</a> .</p> <p><a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/CE_Assembly.tar.gz">CE_Assembly.tar.gz</a> - Centaury referent transcriptome comprises of 160.839 Trinity transcripts grouped in 105.726 Trinity genes.</p> <p><a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/CE_Assembly_fpkm.tar.gz">CE_Assembly_fpkm.tar.gz</a> - fpkm normalized read counts of the assembled transcripts in the six sequenced centaury tissues.</p> <p><a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/nt.db_CE_assembly.tar.gz">nt.db_CE_assembly.tar.gz</a> - annotation of assembled transcripts by mapping them against NCBI nucleotide (NT) database using BLASTn . The obtained results were filtered with E-value E ≤ 10<sup>-3</sup>.</p> <p><a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/swissprot.db_CE_assembly.tar.gz">swissprot.db_CE_assembly.tar.gz</a> - annotation of assembled transcripts by mapping them against NCBI nucleotide (<a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/swissprot.db_CE_assembly.tar.gz">s</a>wissprot) database using BLASTx . The obtained results were filtered with E-value E ≤ 10<sup>-3</sup>.</p> <p><a href="https://zenodo.org/api/files/a0546879-e382-4cf9-8185-f188d1a0c5f0/pfam30.db_CE_assembly.tar.gz">pfam30.db_CE_assembly.tar.gz</a> - annotation of assembled transcripts by mapping them against Pfam30 domain database using hmmer3. The obtained results were filtered with independent E-value E ≤ 10<sup>-3</sup>.</p>
Long-term live imaging and multiscale analysis identify heterogeneity and core principles of epithelial organoid morphogenesis - Image data
<p>The dataset contains raw imaging data from the work:</p> <p>"Long-term live imaging and multiscale analysis identify heterogeneity and core principles of epithelial organoid morphogenesis"</p> <p>The dataset is organized as the following: the "FigureX_" or SupplementaryFigure_X" suffix in the filename refers to the figure in the paper in which the raw data is analyzed and/or visualized. The data is "raw", i.e. not processed. However, in many cases, maximum projections of the original 3D image stacks have been uploaded due to size limitations. The total size of the image stacks approaches 0.5TB. To access the full 3D image stacks please contact the corresponding author (Francesco Pampaloni, fpampalo@bio.uni-frankfurt.de).</p> <p><strong>Authors</strong></p> <p>Lotta Hof<sup>1</sup>*, Till Moreth<sup>1</sup>*, Michael Koch<sup>1</sup>, Tim Liebisch<sup>2</sup>, Marina Kurtz<sup>3</sup>, Julia Tarnick<sup>4</sup>, Susanna M. Lissek<sup>5</sup>, Monique M.A. Verstegen<sup>6</sup>, Luc J.W. van der Laan<sup>6</sup>, Meritxell Huch<sup>7</sup>, Franziska Matthäus<sup>2</sup>, Ernst H.K. Stelzer<sup>1</sup>, Francesco Pampaloni<sup>1§</sup></p> <p><sup>1</sup>Physical Biology Group, Buchmann Institute for Molecular Life Sciences (BMLS), Goethe-Universität Frankfurt am Main, Frankfurt am Main, Germany</p> <p><sup>2</sup>Faculty of Biological Sciences, Goethe-Universität Frankfurt am Main, Frankfurt am Main, Germany</p> <p><sup>3</sup>Department of Physics, Goethe-Universität Frankfurt am Main, Frankfurt am Main, Germany</p> <p><sup>4</sup>Deanery of Biomedical Science, University of Edinburgh, Edinburgh, United Kingdom</p> <p><sup>5</sup>Experimental Medicine and Therapy Research, University of Regensburg, Regensburg, Germany</p> <p><sup>6</sup>Department of Surgery, Erasmus MC – University Medical Center, Rotterdam, The Netherlands</p> <p><sup>7</sup>The Wellcome Trust/CRUK Gurdon Institute, University of Cambridge, Cambridge, United Kingdom. Present address: Max Planck Institute of Molecular Cell Biology and Genetics, Dresden, Germany</p> <p>*contributed equally</p> <p><sup>§</sup>corresponding author: fpampalo@bio.uni-frankfurt.de</p> <p><strong>Abstract</strong></p> <p><em>Background</em></p> <p>Organoids are morphologically heterogeneous three-dimensional cell culture systems and serve as an ideal model for understanding the principles of collective cell behaviour in mammalian organs during development, homeostasis, regeneration and pathogenesis. To investigate the underlying cell organisation principles of organoids, we imaged hundreds of pancreas and cholangio carcinoma organoids in parallel using light sheet and bright field microscopy for up to seven days.</p> <p><em>Results</em></p> <p>We quantified organoid behaviour at single-cell (microscale), individual-organoid (mesoscale), and entire-culture (macroscale) levels. At single-cell resolution, we monitored formation, monolayer polarisation and degeneration, and identified diverse behaviours, including lumen expansion and decline (size oscillation), migration, rotation and multi-organoid fusion. Detailed individual organoid quantifications lead to a mechanical 3D agent-based model. A derived scaling law and simulations support the hypotheses that size oscillations depend on organoid properties and cell division dynamics, which is confirmed by bright field microscopy analysis of entire cultures.</p> <p><em>Conclusion</em></p> <p>Our multiscale analysis provides a systematic picture of the diversity of cell organisation in organoids by identifying and quantifying the core regulatory principles of organoid morphogenesis.</p>
Fig. 1 in Morphology of Two Eschaneustyla Species (Ciliophora, Urostylida), with Notes on Morphogenesis of Eschaneustyla lugeri
Fig. 1. Eschaneustyla terricola (A, B) and E. lugeri (C–E) during interphase, and E. lugeri during morphogenesis (F–L), after protargol impregnation. (A, B) Ventral and dorsal view of same specimen, showing ciliature. Cirri formed from same anlage were connected by solid line. Asterisk denotes the distal end of AZM. (C) Schematic representations of midventral-complex of four E. lugeri specimens with two long midventral rows. Arrows and arrowheads denote midventral rows 1 and 2, respectively. (D, E) Ventral and dorsal view of same specimen, showing typical infraciliature. Cirri formed from same anlage were connected by solid line. Two leftmost cirri develop from anterior part of undulating membranes anlage (dotted line). (F) Ventral view of an early divider that twisted a little at the anterior end, to show the oral primordia of proter (arrow) and opisthe (arrowhead). (G) Enlarged image of proter's oral primordium (arrow) and undulating membranes anlage (arrowhead) of the individual shown F. Note that the former develops in deep of the cortex while the latter develops in the surface. (H) Ventral view of an early divider to show the frontoventral cirral anlagen (arrows). Arrowhead denotes the penultimate frontoventral cirral anlage which forms midventral row 1. Double-arrowhead denotes the frontoventral cirral anlage n that develops into frontoterminal row. Dashed circle represents the flurry area due to the hyperchromatism after protargol impregnation. (I, J) Ventral and dorsal view of an early divider to show the frontoventral cirral anlagen. Arrows and arrowheads in I mark the penultimate and the last frontoventral cirral anlagen, respectively. Note that marginal anlagen and dorsal kineties anlagen (arrows in J) develop intrakinetally. Macronuclear nodules are fusing (arrowheads in J). (K) Ventral view of a middle divider. Arrow marks the partly renewed adoral zone of membranelles of proter. Asterisk denotes two leftmost frontal cirri developed from the undulating membranes anlage. L. Nuclear apparatus of the same specimen as shown in K. Note that macronuclear nodules are fusing into a single mass. AZM, adoral zone of membranelles; CC, caudal cirri; E, endoral; FT, frontoterminal row; LMA, left marginal anlage; LMR, left marginal row; Ma, macronuclear nodules; Mi, micronuclei; MV, midventral row; MV 1, midventral row 1; 1–4, dorsal kineties 1–4; P, paroral; RMA, right marginal anlage; RMR, right marginal row. Scale bars: 100 μm (A, B, D, E); 70 μm (F–L).
Inhibitory G proteins play multiple roles to polarize sensory hair cell morphogenesis
<p>Complete dataset for the manuscript "Inhibitory G proteins play multiple roles to polarize sensory hair cell morphogenesis" including images for illustrations and quantifications. </p>
Data and analysis codes for "In vivo visualization of butterfly scale cell morphogenesis in Vanessa cardui"
<p>Butterfly scale data and data analysis codes for "In vivo visualization of butterfly scale cell morphogenesis in <em>Vanessa cardui</em>."</p> <p> </p> <p>It is recommended to download all files and folders into a single root folder for use in MATLAB.<br> This code was prepared for use in MATLAB R2019b, and some scripts or functions require the Image Processing Toolbox.</p>
Fig. 2 in Comparative Aspects Of The Morphogenesis And Morphology Of The Wing Membranes Of Bats (Сhiroptera) And Flying Lemurs (Dermoptera)
Fig. 2. Hand and wing membrane of embryo Cynocephalus variegatus, stage 20. Longitudinal sections. The right forearm. А, D, E, F — x400; B, C — x1000: А — longitudinal (below) and cross-section (from above) of the propatagium skin; B, C — the muscle tubes in the plagiopatagium skin; D — the two row of muscle tubes in the plagiopatagium skin; E, F — the chiropatagium skin. Epidermis (ЕPD), undifferentiated mesenchyme (М), blood vessel and blood capillaries (V and CAP), muscle tubes (MT), muscles (MUS), rudiments of digits I (I) and II (II); IV (IV) and V (V).Stained with Mallory's trichrome.
Fig. 1 in Comparative Aspects Of The Morphogenesis And Morphology Of The Wing Membranes Of Bats (Сhiroptera) And Flying Lemurs (Dermoptera)
Fig. 1. Hand and wing membrane of bats embryos. А, B, C — x400; D — x1000: А — embryo Myotis blythii stage 18. Longitudinal section. The left forelimb bud with metacarpals rudiments: mesenchymal condensations of metacarpal rudiments (Mc), undifferentiated mesenchime (M), epidermis (EPD). Stained with Ehrlich's hematoxylin and eosin; В — embryo Rhinolophus hipposideros stage 20. Cross-section. The wing membrain (uropatagium). The centre of hemopoiesis (G), epidermis (ЕPD), undifferentiated mesenchyme (М), blood vessels (V). Stained with Mallory's trichrome; C — embryo Myotis blythii stage 19. Longitudinal section. The right forearm. Metacarpal rudiments (Mc), digits rudiments (II III, IV, V), epidermis (ЕPD), undifferentiated mesenchyme (М), blood vessels (V). Stained with Ehrlich's hematoxylin and eosin; D — embryo Myotis blythii stage 22. Cross-section of the plagiopatagium skin. The centre of hemopoiesis (G), mesenchyme (М), epidermis (ЕPD). Stained with Ehrlich's hematoxylin and eosin.
Dataset and software to analyze and simulate neuronal morphogenesis in Drosophila class IV da neurons
<p>The highly ramified arbors of neuronal dendrites provide the substrate for the high connectivity and computational power of the brain. Altered dendritic morphology is associated with neuronal diseases. Many molecules have been shown to play crucial roles in shaping and maintaining dendrite morphology. Yet, the underlying principles by which molecular interactions generate branched morphologies are not understood. To elucidate these principles, we visualized the growth of dendrites throughout larval development of Drosophila sensory neurons and discovered that the tips of dendrites undergo dynamic instability, transitioning rapidly and stochastically between growing, shrinking, and paused states. By incorporating these measured dynamics into a novel, agent-based computational model, we showed that the complex and highly variable dendritic morphologies of these cells are a consequence of the stochastic dynamics of their dendrite tips. These principles may generalize to branching of other neuronal cell-types, as well as to branching at the subcellular and tissue levels.</p>
Data from: The roles of growth regulation and appendage patterning genes in the morphogenesis of treehopper pronota
<p>Treehoppers of the insect family Membracidae have evolved enlarged and elaborate pronotal structures, which is hypothesized to involve co-opted expression of genes that are shared with the wings. Here, we investigate the similarity between the pronotum and wings in relation to growth. We show that the ontogenetic allometry of the pronotum is similar to that of wings in Membracidae, but not the outgroup. Using transcriptomics, we find genes related to protein synthesis and translation are mutually upregulated. These genes are implicated in the eIF2, eIF4/p70S6K, and mTOR pathways, and have known roles in regulating cell growth and proliferation. We show that species-specific differential growth patterning of the pronotum begins as early as the third instar. This finding suggests that co-option of appendage patterning genes must occur before the metamorphic molt. We propose that a network related to growth and size determination is the more likely mechanism shared with wings. However, regulators upstream of the shared genes in the pronotum and wings need to be elucidated to substantiate whether co-option has occurred. Finally, we<span> believe it will be helpful to distinguish the mechanisms leading to pronotal size from those regulating pronotal shape as we make sense of this spectacular evolutionary innovation. </span></p>
Fig. 2 in Morphology of Two Eschaneustyla Species (Ciliophora, Urostylida), with Notes on Morphogenesis of Eschaneustyla lugeri
Fig. 2. Photomicrographs of Eschaneustyla lugeri (A, B) and E. terricola (D, E) in life and E. lugeri after protargol impregnation (C, F–M). (A, B) Representative individuals. Arrow in A denotes the contractile vacuole. (C) Dorsal side to show the arrangement of extrusomes (arrows). (D) Arrangement of cortical granules. (E) Ventral view. Arrow marks the contractile vacuole. It should be noted that the specimen in E is slightly damaged, thus it doesn't present a narrowly rounded posterior end. (F–H) Ventral views of early dividers, to show the oral primordia of opisthe (F) and proter (arrow in G), the undulating membranes anlage (arrowhead in H) and the frontoventral cirral anlagen (arrow in H). (I) Dorsal view of an early divider to show the intrakinetal development of dorsal kineties anlagen (arrows). (J) Fusion of macronuclear nodules. (K–M) Ventral views of middle dividers. Note that right marginal anlage develops intrakinetally (arrow in K). Arrow in L denotes the formation of the leftmost frontal cirri from frontoventral cirral anlage I. In M, arrow marks the frontoventral cirral anlage n that becomes the frontoterminal row and arrowhead depicts the penultimate frontoventral cirral anlage that forms midventral row 1, respectively. Ma, macronuclear nodules. Scale bars: 100 μm (A, B, E); 40 μm (C, F, G, I); 15 μm (D, J); 25 μm (H, K–M).
Figure 5 in Morphogenesis of Ulva mutabilis (Chlorophyta) induced by Maribacter species (Bacteroidetes, Flavobacteriaceae)
Figure 5: Phylogenetic tree of strains of Flavobacteriaceae tested for morphogenetic activities. Maximum Likelihood (ML) phylogenetic inference of 16S rRNA gene sequences of the genus Maribacter and related genera in the family Flavobacteriaceae (phylum Bacteroidetes). Maribacter sp. strain MS6 (bold) and all type strains found to be MS6 substitutes in Ulva morphogenesis bioassays are marked in green. Test type strains which did not elicit the MS6 morphotype are marked in dark-red. For taxonomic robustness, the tree was constructed only with high-quality, ≥ 1300 bp 16S rRNA gene sequences, mostly from type strains. The gene sequence of strain MBIC04683 (349 bp) was added to the tree a posteriori using the ARB parsimony function. Numbers at tree nodes are bootstrap values calculated in ML analysis, and values ≥ 70% are shown. The unrooted tree is drawn to scale, and the scale bar represents the number of nucleotide substitutions per site (Costa et al. 2013, Keller-Costa et al. 2014). Arrows indicate strains which were identified as morphogenesis-inducing bacteria in previous studies (Matsuo et al. 2003, Spoerner et al. 2012).
Figure 4 in Morphogenesis of Ulva mutabilis (Chlorophyta) induced by Maribacter species (Bacteroidetes, Flavobacteriaceae)
Figure 4: Relative morphogenetic activity of the tested Flavobacteriaceae. Algae with normal cell wall formation (i.e. without any protrusions) were counted after 14 days of co-cultivation with following bacterial type strains: Maribacter chUngangensis, Maribacter arcticUs, Maribacter sedimenticola, Maribacter stanieri, Maribacter Ulvicola, Maribacter polysiphoniae, Algibacter lectUs, Ulvibacter litoralis, Polaribacter dokdonensis, PseUdozobellia thermophila, Arenibacter palladensis, MUricaUda zhangzhoUensis and the isolated strains RoseovariUs sp. MS2 (formerly Roseobacter sp. MS2) and Maribacter sp. MS6 (formerly Cytophaga sp. MS6). Error bars represent standard deviation (n = 50–70 individual algae). RoseovariUs sp. MS2 and Maribacter sp. MS6 were used as control strains for comparison.
Figure 1 in Morphogenesis of Ulva mutabilis (Chlorophyta) induced by Maribacter species (Bacteroidetes, Flavobacteriaceae)
Figure 1: Control experiment for complementary activity of morphogenesis-inducing bacteria (reference strains). Axenic Ulva mUtabilis sl G mt(+) germlings (A) were inoculated with either RoseovariUs sp. MS2 (B) or Maribacter sp. MS6 (C) or both bacteria (D). Gametophytes were propagated for gamete production and release under laboratory conditions (Wichard and Oertel 2010). Afterwards axenic gametes were prepared according to Wichard (2015). Purified gametes [mating type (+)] were inoculated with selected bacteria (final concentration OD = 1 × 10 − 6) in 10 ml Ulva culture medium and kept in the dark for 24 h to let gametes settle on culture tissue flask. After 14 days 600 growth at 18°C and 90–120 µmol photons s− 1 m− 2 for 17 h light and 7 h dark, thallus development of 50–70 germlings derived from triplicate experiments was examined with an inverted Leica DMIL LED microscope (Leica, Solms, Germany) equipped with a digital camera (Nikon, Düsseldorf, Germany). The four morphotypes are colour-coded. Black arrows indicate protrusions from the exterior cell wall. Scale bars = 100 µm.
Figure 3 in Morphogenesis of Ulva mutabilis (Chlorophyta) induced by Maribacter species (Bacteroidetes, Flavobacteriaceae)
Figure 3: Bioassay screening for morphogenetic activity among selected Flavobacteriaceae (rows). Two-week old germlings are shown. Selected strains were tested with axenic Ulva gametes alone (left column: A–F) and in combination with RoseovariUs sp. MS2 (middle column: G–L) or with Maribacter sp. MS6 (right column: M–R). Black arrows indicate protrusions from the exterior cell wall. Different colours of frames indicate different morphotypes, as explained in Figure 2 and shown for the control experiments in Figure 1. Scale bars = 100 µm.
Figure 2 in Morphogenesis of Ulva mutabilis (Chlorophyta) induced by Maribacter species (Bacteroidetes, Flavobacteriaceae)
Figure 2: Bioassay screening for morphogenetic activity among selected Maribacter strains (rows). Two-week old germlings are shown. Maribacter strains were tested with axenic Ulva gametes alone (left column: A–F) and in combination with RoseovariUs sp. MS2 (middle column: G–L) or with Maribacter sp. MS6 (right column: M–R). Yellow framing (F) highlights an axenic-like development and morphotype with protrusions from the exterior cell wall (black arrow). Purple framing (L) shows cell divisions and blade formation with malformed cell walls (black arrow) indicating an MS2-like morphotype. Red framing (A–E, M–R) shows longitudinal growth and normal cell wall formation similar to the MS6-like morphotype. If the tested strain harboured an MS6-like bioactivity and was inoculated with RoseovariUs sp. MS2, the complete morphogenesis was observed (green framing, G–K). Scale bars = 100 µm.
Fig. 8. A–H in A Huge Diversity of Metopids (Ciliophora, Armophorea) in Soil from the Murray River Floodplain, Australia. II. Morphology and Morphogenesis of Lepidometopus platycephalus nov. gen., nov. spec.
Fig. 8. A–H. Lepidometopus platycephalus, ciliary pattern and nuclear apparatus of a late divider (A, B), early post-dividers (C–F), and a late post-divider (G, H) in protargol preparations. Arrowheads in (A, B) mark barren area that forms at the posterior end of the proter and at the anterior end of the opisthe after the parental somatic ciliary rows split in the middle. Dashed lines in (D, F) delimit the flattened anterior body portion, i.e., the preoral dome. AZP – adoral zone of polykinetids; CP – cytopharynx; CV – contractile vacuole; MA – macronucleus; MI – micronucleus; OAZP – opisthe's adoral zone of polykinetids; OPM – opisthe's paroral membrane; OPS – opisthe's perizonal stripe; PAZP – proter's adoral zone of polykinetids; PD – preoral dome; PM – paroral membrane; PPM – proter's paroral membrane; PPS – proter's perizonal stripe; PS – perizonal stripe; SK – somatic kineties. Scale bars: 20 µm.
Fig. 5. A–E in A Huge Diversity of Metopids (Ciliophora, Armophorea) in Soil from the Murray River Floodplain, Australia. II. Morphology and Morphogenesis of Lepidometopus platycephalus nov. gen., nov. spec.
Fig. 5. A–E. Lepidometopus platycephalus in the SEM. A. Epicortical scales (lepidosomes). B. Left side overview, showing the strongly flattened preoral dome (asterisk). C. Oblique posterior polar view, showing the globular postoral portion roofed by the cap-shaped preoral dome. D. Detail of oral area, showing the tongue-like paroral membrane and the adoral zone of polykinetids whose cilia spread backwards. The dome lip is very narrow while the side stripe forms a rather deep channel covered with epicortical scales. E. Ventrolateral view of oral body portion. The arrowhead marks entrance to buccal cavity. This cell lost lepidosomes during the preparation process. AC – adoral cilia; DL – dome lip; PD – preoral dome; PM – paroral membrane; PS – perizonal stripe; SC – somatic cilia; SS – side stripe. Scale bars: 1 µm (A), 5 µm (D, E), and 20 µm (B, C).
Fig. 6. A–J in A Huge Diversity of Metopids (Ciliophora, Armophorea) in Soil from the Murray River Floodplain, Australia. II. Morphology and Morphogenesis of Lepidometopus platycephalus nov. gen., nov. spec.
Fig. 6. A–J. Lepidometopus platycephalus, ciliary pattern and nuclear apparatus of early dividers (A–H) and of an early mid-divider (I, J) after protargol impregnation. Arrowheads mark the prospective adoral polykinetids formed at the posterior end of dorsal and dorsolateral kineties. Asterisks denote the prospective adoral polykinetids developing at the anterior end of the postoral kineties. Arrow in (I) points to two dorsolateral kineties which migrate towards the growing perizonal stripe to become perizonal rows 4' and 5' in the opisthe. BU – bulge; CV – contractile vacuole; MA – macronucleus; MI – dividing micronucleus; OAZP – opisthe's adoral zone of polykinetids; PAZP – proter's adoral zone of polykinetids; PM – paroral membrane; PPS – proter's perizonal stripe. Scale bars: 20 µm.
Fig. 7. A–F in A Huge Diversity of Metopids (Ciliophora, Armophorea) in Soil from the Murray River Floodplain, Australia. II. Morphology and Morphogenesis of Lepidometopus platycephalus nov. gen., nov. spec.
Fig. 7. A–F. Lepidometopus platycephalus, ciliary pattern and nuclear apparatus of mid-dividers after protargol impregnation. Asterisks denote scattered dikinetids of perizonal rows 1 and 2 that migrate along the new adoral zone to assemble the opisthe's paroral membrane. Arrows point to two dorsolateral kineties which migrate towards the opisthe's perizonal stripe to become rows 4' and 5'. Arrowheads mark newly formed ciliary rows left of opisthe's adoral zone. CH – chromosomes; F – fibres; MA – macronucleus; MI – micronucleus; OAZP – opisthe's adoral zone; OPM – opisthe's paroral membrane; PAZP – proter's adoral zone; PD – preoral dome; PPM – proter's paroral membrane; PS – perizonal stripe rows. Scale bars: 20 µm.
Fig. 4. A–J in A Huge Diversity of Metopids (Ciliophora, Armophorea) in Soil from the Murray River Floodplain, Australia. II. Morphology and Morphogenesis of Lepidometopus platycephalus nov. gen., nov. spec.
Fig. 4. A–J. Lepidometopus platycephalus in the SEM. A–E. Ventral (A), right side (B), dorsolateral (C, D), and left side (E) overview, showing general body organization. Opposed arrowheads mark the strongly flattened distal portion of the preoral dome (B, E); arrows denote left side cilia (B–D). F. Ventrolateral view, showing the paroral membrane and the perizonal stripe. G. Dorsolateral view, showing five perizonal rows. H. Epicortical scales. I, J. Only a single basal body is ciliated in the postoral dikinetids (I) except for the left side kineties where both basal bodies are ciliated (J). (1–5) – perizonal rows; AZP – adoral zone of polykinetids; PD – preoral dome; PM – paroral membrane; PS – perizonal stripe; SC – somatic cilia. Scale bars: 1 µm (H), 2 µm (G), 3 µm (F), 5 µm (I, J), and 20 µm (A–E).
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.