The evolution of specific appendages is made possible by the ontogenetic deployment of general cell signaling pathways. Many fishes, amphibians and reptiles have unique skin appendages known as barbels, which are poorly understood at the cellular and molecular level. In this study, we examine the cell arrangements, cell division patterns, and gene expression profiles associated with the zebrafish maxillary barbel, or ZMB. The earliest cellular organization of the ZMB is an internal whorl of mesenchymal cells in the dermis of the maxilla; there is no epithelial placode, nor any axially-elongated epithelial cells as expected of an apical ectodermal ridge (AER). As the ZMB develops, cells in S-phase are at first distributed randomly throughout the appendage, gradually transitioning to a proliferative population concentrated at the distal end. By observing ZMB ontogenetic stages in a Wnt-responsive transgenic reporter line, TCF siam, we identified a strongly fluorescent mesenchymal cell layer within these developing appendages.

• Vwr 1530 Incubator Manual
• Vwr Incubator Model 2325 Manual Transmission Diagram
• Vwr Incubator Model 2325 Manual Transmission Fluid

Fisher Scientific13K Microcentricfuge Users Manual Forma Countertop Incubator Model 3029/3039 Forma Refrigerated Console Incubator Orbital Shaker Model 4580/4581 FOCI Spectrofluorometers for Fluorescence Spectroscopy 190-900 Nanometers Forma Baths and Circulators Models 2352, 2376, 2112, 2121, 2135, 2095, 2161, 2006, 2067, 2325, 2425. VWR Forced Air incubators provide an even higher temperature uniformity and stability for reproducible results in microbiology and research labs.Maintaining a controlled environment for cell cultures and microorganisms, the standard incubators will grow organisms and store sensitive samples. Glycine receptors (GlyR) belong to the pentameric ligand-gated ion channel (pLGIC) superfamily and mediate fast inhibitory transmission in the. Cells were plated on poly-l-lysine-coated glass coverslips (Sigma and VWR, respectively) in 35-mm culture dishes (Scientific Laboratory Supplies, SLS).

Using an in vitro explant culture technique on developing barbel tissues, we co-localized the fluorescent label in these cells with the mitotic marker EdU. Surprisingly, TCF+ cells showed little proliferation, indicating a slow-cycling subpopulation.

Transmission electron microscopy of the ZMB located the TCF+ cells in a single, circumferential layer within the barbel’s matrix core. Morphologically, these cells resemble fibroblasts or osteoblasts; in addition to their matrix-bound location, they are identified by their pancake-shaped nuclei, abundant rough endoplasmic reticulum, and cytoplasmic extensions into the surrounding extracellular matrix. Taken together, these features define a novel mesenchymal cell population in zebrafish, the ‘TCF+ core cells.’ A working model of barbel development is proposed, in which these minimally mitotic mesodermal cells produce collagenous matrix in response to ectodermally-derived Wnt signals deployed in a proximal-distal gradient along the appendage.

This documents a novel mechanism of vertebrate appendage outgrowth. Similar genetic signals and cell behaviors may be responsible for the independent and repeated evolution of barbel structures in other fish species.

Introduction Skin is the boundary between an animal and its environment. At this interface, vertebrates have evolved many specialized appendages including scales, fins, teeth, feathers, and hair (;;; ). Although anatomically and functionally diverse, all of these structures arise from local interactions between two layers of cells: the epidermis and the dermis. Understanding epidermal-dermal interactions at the cellular and molecular levels is of interest for three reasons. Firstly, knowing how skin appendages develop may allow us to infer which are homologous, and how these appendages evolved from those of common ancestors. Secondly, the developmental mechanisms of appendage outgrowth are the ultimate source of appendage variation, including ontogenetic stages, sexual dimorphisms, or individual phenotypes.

Finally, many of the cellular behaviors observed during appendage ontogeny, including cell proliferation, cell migration, and changes in gene expression, are re-used when appendages undergo wound healing or regeneration (;;;; ). Therefore the study of epidermal-dermal interactions in the context of appendage development advances at least three inter-related fields simultaneously– those of phylogeny, ontogeny, and physiology. Of the living vertebrates, fishes have some of the most diverse skin appendages.

Within bony fishes, several species are intensively studied, including the zebrafish, medaka, and stickleback. In zebrafish, skin appendages include pharyngeal teeth , elasmoid scales , the lateral line (;; ), several unpaired fins , and the nasal and maxillary barbels (; ). Among these, the mechanisms of barbel development are of special interest due to the morphological diversity of these structures, temporal variation in their ontogenetic appearance, and multiple gains and losses in fish evolutionary history. Compares the barbels of two fishes, the zebrafish ( Danio rerio) and the channel catfish ( Ictalurus punctatus). Each fish has a different anatomical arrangement of facial barbels (two pairs vs. Four), which appear at different stages of development (juvenile vs. Histologically, these appendages contain overlapping, but not identical cell types; catfish barbels are supported by cartilaginous rods, whereas zebrafish barbels are not (; ).

This unique pattern leads to questions of both ontogenetic and phylogenetic processes. Specifically, how do the ectodermal and mesodermal layers of fish skin accomplish the localized extension of these elongated appendages? How often have certain developmental mechanisms been used, within bony fishes, to accomplish so many massively parallel adaptive events?

Evolutionary and developmental context of barbel development in several species of ray-finned fishes (Actinopterygii) Wnt proteins are highly conserved extracellular ligands that drive many ontogenetic processes, including skin appendage development (Logan and Nusse, 2004;; Chien et al., 2009). Canonical Wnt signaling causes cytoplasmic stabilization and nuclear localization of β-catenin, activating gene transcription through T-cell factor/lymphoid enhancer factor (TCF/LEF) proteins (MacDonald et al., 2009.) Through a different network of cytoplasmic events, Wnts can also signal non-canonically. Experiments in avian and mammalian models have shown that both canonical and non-canonical Wnt signaling have highly conserved roles in dermal differentiation, epidermal-dermal induction, and skin appendage patterning (Huelsken et al., 2001; Andl et al., 2002; Rinn et al., 2008;; Mikkola, 2007; ). For example, if extracellular inhibitors of Wnt binding are overexpressed in the epidermis or dermis, abnormal skin and arrested appendages can result (; ). Likewise, disrupting the intracellular components of canonical Wnt signaling, including adenomatous polyposis coli (APC, Kuraguchi et al., 2006), β-catenin (Huelsken et al., 2001), or TCF/LEFs (Niemann et al., 2002; van Genderen et al., 1994) can also cause skin anomalies.

We therefore predicted that Wnt signaling might have a primary role in establishing and maintaining the zebrafish maxillary barbel, affecting dermal cell proliferation and/or matrix production during barbel ontogeny. Although there has been one recent molecular survey on the ontogeny of catfish barbels , there are no comparable studies for similar structures in zebrafish. To better understand how the maxillary barbel develops, our goal was to study cell shape, cell proliferation and gene expression during outgrowth of this appendage. Our results suggest that, in contrast to other vertebrate appendages, the maxillary barbel forms without any corresponding ectodermal placode or apical ectodermal ridge (AER). Cell division in the developing barbel is also haphazard, showing no localized growth zones. In contrast, we detected a strongly labeled, single-layered subpopulation of TCF-responsive cells within the barbel core.

The fluorescent labeling of these cells had a very strong proximal-distal gradient, with maximal signal distally, that was maintained from the juvenile to the adult. Further studies confirmed that these cells, which have not previously been described, were minimally mitotic, but could be uniquely identified by their matrix-bound location, nuclear morphology and cytoplasmic structure. We conclude that we have identified a new cell population in zebrafish, here called the ‘TCF+ core cells’, which may be responsive to canonical Wnt signals.

Importantly, this dermal population is uniquely placed to contribute to maxillary barbel outgrowth through enhanced extracellular matrix production. Fish lines and husbandry Three zebrafish strains were used in this study: a wildtype AB strain (ZDB-GENO-960809-7), a transgenic strain expressing membrane-bound green fluorescent protein (Tg(Ola.Actb:Hsa.HRAS-EGFP); ZDB-GENO-061107-1 , and a transgenic strain expressing a TCF-responsive nuclear-localized mCherry, an indicator of canonical Wnt signaling (Tg(7xTCF-Xla.Sia:NLS-mCherry); ZDB-GENO-110113-3. These strains are hereafter called wild type, mGFP, and TCF siam, respectively. DePaul University’s Institutional Animal Care and Use Committee (IACUC) approved all experimental protocols. Juvenile and adult zebrafish were housed in a recirculating system filled with dechlorinated tap water (pH 7.4) at 28–29°C.

Light was provided on a 14 hr:10 hr day:night cycle. Sexually mature adults were pair-bred in crossing tanks and fertile eggs collected using standard methods. 6–7 days after hatching, embryos were transferred to 200 mL static tanks in a 28°C incubator and fed live rotifers and/or larval powder twice daily (Larval Diet LD100; Aquatic Ecosystems). When of sufficient size, larvae were moved to tanks in the recirculating rack and fed live brine shrimp and/or commercial fish flakes (TetraMin Tropical Flakes) for the remainder of the study. For all surgical procedures, fish were anaesthetized in 0.015% Tricaine (MS-222, Fisher Scientific: AC) buffered to pH 7.0 in system water. For euthanasia, fully anesthetized fish were submerged in ice water until opercular movements were no longer observed.

Developmental staging and tissue collection Although there is a single nomenclature for zebrafish embryonic development , there are multiple proposed systems for juveniles and adults (; ). Postembryonic staging can be complex because there are more structures to observe, as well as increased variability among structures. In this study, we used a simple, straight-line distance measure, standard length.

This variable is rapidly measured, and the relationship between standard length and barbel length has already been mapped in a large (n 100) series of wildtype zebrafish juveniles. Because these two morphological variables are strongly correlated, either measure can be used to indicate relative developmental stage. To obtain a complete developmental series of maxillary barbels including pre-barbels, barbel buds and early-elongating appendages, wildtype and mGFP juveniles were collected at intervals from 4–8 weeks post-fertilization. After euthanasia, they were fixed whole in either Dent’s fixative (80% methanol: 20% DMSO) or 4% paraformaldehyde in phosphate-buffered saline (PF-PBS, pH 7.4) for 2–4 hours at room temperature or overnight at 4°C. After fixation, the specimens were rinsed in 1x phosphate buffered saline (PBS) and each fish was measured under a dissecting microscope from the anteriormost tip of the lower jaw to the posteriormost margin of the trunk musculature along the central axis of the caudal fin.

Each fish was then sorted into one of four arbitrary body size classes: 1) pre-barbels (SL 15 mm). Both maxillary barbels were then dissected off for immediate processing, or dehydrated to 100% methanol for storage at −20°C. In vitro EdU labeling of zebrafish tissue explants To identify cells in S-phase during maxillary barbel development, we developed a method for whole-mount EdU labeling of zebrafish tissue explants in vitro. This protocol was adapted from prior studies using EdU to label cell proliferation in whole chick embryos and isolated Drosophila brains. As a positive control for successful mitotic labeling, we also cultured explants of the regenerating adult caudal fin, as its patterns of in vivo cell proliferation have been well described (; ). A detailed description of our control and experimental treatments is given below. To prepare the control tissue, we excised the distal caudal fins from groups of 6 adult wildtype fish on each of 4 consecutive days, designated days 3, 2, 1 and 0.

Fish prepared on days 3, 2 and 1 were returned to the recirculating system and allowed to regenerate until day 0 tissue collection. Fish prepared on day 0 were collected while still anaesthetized, immediately after the tail excision surgery.

Overall, 24 adult tails were examined. Also on day 0, we collected 12 wildtype siblings. These fish had standard lengths of 10–15 mm, and each provided two maxillary barbels in various stages of development, for a total of 24 barbel appendages.

Using sterile technique in a flow-through biocontainment hood, the regenerating blastemas of the adult tails and the maxillary barbels of the juveniles were dissected off and placed, 2–3 tissue pieces per well, in a 48-well plastic tissue culture plate. Each experimental well held 200 μL of pre-warmed (28°C) sterile Leibovitz-15 culture media (pH 7.4; VWR: 89222-116), supplemented with 3% fetal bovine serum (FBS) and antibiotics (100 U/mL penicillin and 100 ug/mL streptomycin). This mixture was called ‘complete L-15’. Next, a 2x working solution of EdU was freshly prepared by thoroughly mixing 1 part EdU stock solution (10 mM) with 98 parts complete L-15 and 1 part DMSO (= 1000 μM EdU, 1% DMSO). Finally, 200 μL of this 2x EdU solution was added to each experimental well holding the tissue. The final volume in each well was therefore 400 μL, and the final concentration was 500 μM EdU: 0.5% DMSO. As a negative control, the EdU working solution was not added to several experimental wells containing either barbel or tail tissue.

To allow EdU uptake, the covered, sterile plate was placed in a dark, humidified air incubator (28°C) for 4 hours. After this interval, most of the solution in each well was carefully removed from around the tissue fragments with a P-1000 pipettor and a narrow gel-loading tip.

Each well was then washed two times with 0.5 mL of 1x PBS. Finally, 0.5 mL of freshly thawed 4% PF-PBS fixative was added to each well and the plate was placed at 4°C overnight. Whole-mount detection of the EdU-labeled explants followed the manufacturer’s instructions (Click-iT EdU Imaging Kit, Invitrogen: ). The fixed tissues in each well were washed 2–3 times in 0.5 mL blocking buffer (3% BSA in PBS), soaked 1 hour in 0.5 mL permeabilization buffer (1x PBS + 0.5% Triton-X), and rinsed 2–3 times in 0.5 mL blocking buffer. After excess wash was removed, 300 μL of freshly prepared ‘Click-iT’ reaction mix was added to each well. In this step, copper-catalyzed ‘click’ reaction occurs in which a fluorophore-conjugated azide binds irreversibly to an alkyne group of EdU.

To insure adequate mixing during this light-sensitive step, the plate was wrapped in foil and gently agitated on a titer-plate shaker for 30 minutes at room temperature. The reaction cocktail was then removed. After two washes in 0.5 mL blocking buffer and one wash in 0.5 mL PBS, nuclei were then counterstained by adding 250 μL of Hoechst 33342 solution to the PBS in each well (final concentration = 5 μg/mL).

After another 30 minutes of agitation in the dark, excess Hoechst was removed by 2–3 additional PBS rinses. Finally, the tissue fragments were pipetted out of the wells, cleared in 70% glycerol, mounted on microscope slides and imaged using confocal microscopy. Emission/excitation wavelengths were 590/615 nm for the EdU fluorophore (Alexa Fluor 594) and 350/461 nm for the Hoechst nuclear label, respectively.

Microscopy, photography, image processing and video formatting To detect and colocalize fluorescent signals, tissue samples were examined using an epifluorescent microscope (Nikon Eclipse 50i) and/or a laser scanning confocal (Leica Microsystems SPE; Model # DMI4000). Images were exported and archived as individual TIF files. Single TIFs were processed in Adobe Photoshop CS5 using standard tools to adjust image sharpness, brightness, and contrast.

Z-stacks of TIFs were imported into FluoRender, a free confocal imaging program , and three-dimensionally rendered using the software tools available. Step-by step Fluorender workflow protocols are available on request.

To produce animations, rendered images series were exported from Fluorender as JPEG files and assembled into annotated movies using Movavi Video Suite. Barbel outgrowth: changes in cell shape and distribution Skin appendage morphogenesis involves regulated cell rearrangements of both epithelium and mesenchyme Certain embryonic structures are found repeatedly in vertebrate ontogeny, and represent current archetypes of how appendages are organized. Examples include epithelial placodes, which are important for the location of superficial structures such as hair, teeth, feather tracts and sensory ganglia (;;; ) and apical ectoderm ridges (AERs), which are found on developing tetrapod limb buds and fish fins (;;; ). In this study, we used transgenic zebrafish expressing membrane-bound green fluorescent protein (mGFP) to observe changes in cell shape and distribution during ZMB morphogenesis. GFP expression in this line is randomly mosaic; for these experiments, fish lines were screened for strong expression in the epidermis, as opposed to the dermis. This allowed us to distinguish the two layers, and, in combination with nuclear staining, observe the general shape and distribution of epidermal cells.

Specifically, we sought to identify any epithelial reorganization, such as a placode or ridge, which would precede barbel outgrowth. Forty-eight mGFP zebrafish were sorted into four categories of standard length (SL): 15 mm SL (n = 6).

Budding of the ZMB is first observed at approximately 10 mm SL; therefore, the majority of specimens were at this stage or earlier. In juvenile zebrafish without external protrusions of the barbels (SL 1 mm long), the epidermal cells form a stratified cuboidal epithelium with 3–4 layers of cells throughout, as previously described. At no stage did we observe any local thickening of the epidermis, typical of an epithelial placode, nor any collection of distally elongated epithelial cells, characteristic of an AER. Barbel outgrowth: patterns of cell proliferation Appendage outgrowth is the net result of cell distribution and cell proliferation. Cell proliferation is required for organized growth; however, there are different spatial patterns in which proliferation occurs. An apical model predicts that the most distal cells will divide most rapidly, , whereas a basal model predicts the opposite.

A distinct sub-apical region of concentrated cell division can be called a “progress zone” ; alternatively, or cell divisions can be spatially random. Each patterns of proliferation suggests a corresponding distribution of developmental signals locally controlling the cell cycle. To analyze cell proliferation in the developing ZMB, we collected barbel tissues from three body size classes (10–12.5, 12.5–15, and 15 mm SL) and explanted them for 4 hours in a sterile culture medium containing EdU (see Methods).

After detection, we were able to map the labeled cells in this outgrowing structure, a phenomenon not previously described. Similarly-treated positive control tissues (the distal ends of regenerating adult caudal fins) were also successfully labeled, showing intense signal in nuclei of the blastema (not shown). In early-developing maxillary barbels (10–12.5 mm SL) we saw scattered EdU labeling in both epithelial and mesenchymal layers throughout the appendage.

These labeled cells had a haphazard or random pattern. Similarly, barbels from slightly more developed fish (12.5–15 mm SL) had both proximal and distal regions labeled with dispersed, EdU-positive cells. We noted slightly increased mitotic labeling on the ventral surface of the barbel, where there are numerous epithelial taste-bud clusters.

In the largest barbels examined (15 mm SL), this dispersed pattern of cell labeling was essentially unchanged. Overall, the gross morphology of the cultured explants appeared excellent, and optical sectioning of the stained specimens showed bright, crisp nuclear labeling in both superficial and deep cell populations. This indicates that, during the 4-hour culture period, a large number of cells remained viable and were able to complete S-phase. Further, it shows that the EdU label effectively penetrated the skin and basement membrane, even in the absence of physiological circulation or mechanical fluid mixing.

A Wnt/TCF reporter line labels a subset of ZMB core cells Wnt signaling is crucial for many developmental processes, but particularly dermal differentiation (; ). Several zebrafish lines have been engineered to express fluorescent reporters downstream of Wnt pathway activation (; ). Of these, we chose the recently-developed TCF siam:mCherry line, which provides a readout of canonical Wnt signaling, through TCF activity in affected nuclei. This line faithfully mimics all known embryonic Wnt signaling domains; however, there are no studies using this line in juveniles or adults. By observing this line at various stages of barbel outgrowth, we sought to detect any local activation of this key genetic pathway. We raised hemizygous TCF siam zebrafish to adulthood and outcrossed them to wild types.

At 24 hours post-fertilization, we screened the progeny for strong mCherry expression in the tailbud nuclei, a known domain of Wnt activity. All confirmed mCherry + transgenics were then allowed to grow for at least 4 weeks prior to collection, screening, and counterstaining of the maxillary barbel tissue. Juvenile TCF siam zebrafish had strong nuclear mCherry in cells of the olfactory pit, mandibular cartilage, and maxillary barbel bud. Magnification of the bud domain showed several dozen mCherry + nuclei arranged in a cone-shaped sleeve over the barbel core. At later stages of barbel outgrowth, a similar distribution of nuclei was observed within the distal two-thirds of the appendage.

In adult maxillary barbels, there was little or no fluorescent signal along the barbel shaft; however, a strongly-labeled subpopulation remained at the distal end. Volume rendering showed that, at all stages examined, the mCherry + nuclei were radially flattened, circumferentially distributed, and occupied a single, sub-epidermal layer (, and ). These signals identify a novel subpopulation of maxillary barbel cells that is continuously responsive to TCF, a component of canonical Wnt signaling. These cells are present from the early bud stage to the adult appendage. TCF+ cells of the ZMB are not highly mitotic Wnt ligands can have multiple cellular effects, inducing coordinated changes in gene expression, cell morphology and behavior. Having identified the TCF + core cells by their reporter gene activity, we next wanted to understand their mitotic behavior. Specifically, we wished to explore if these were rapidly-cycling cells that might provide a pool of undifferentiated precursors to the developing appendage.

To test this, we repeated our in vitro EdU-labeling technique on freshly explanted barbel tissues from this transgenic line. In these experiments, the dissection and labeling procedures were identical to those previously performed, except that EdU detection was performed with an AlexaFluor 488-conjugated azide, staining S-phase nuclei green. All double-labeled cells (mCherry+/488+) would indicate TCF+ cells that were also in S-phase during the 4-hour labeling interval. Confocal imaging of the stained, transgenic barbels confirmed a single, deep layer of mCherry+ nuclei circumferentially arranged around the central core. We also detected intense EdU labeling in many cells, but most of these were green-only and were more superficially located.

These abundant, superficial EdU+ cells likely represent basal epithelial cells, a rapidly-dividing subpopulation of the epidermis. Some of the mCherry+ cells were double-labeled (mCherry+/EdU+, ); however, these were a small minority of the total population. We conclude that the TCF+ barbel cells have some mitotic activity during the stages examined. However, relative to surrounding cells, they infrequently divide. Ultrastructure of the TCF+ core cells Using nuclear-localized reporter genes and mitotic staining methods, we identified a TCF+, slow-dividing cell population within the ZMB.

This nuclear staining alone, however, did not provide a complete picture of this new cell type or its developmental role. As previously described, ZMB extension involves the accumulation of dense, non-mineralized matrix fibers within the dermal core of the appendage. These condense to form the central rod, which is the anatomical supporting structure and mechanical lever arm for the appendage Histologically, the central rod appears largely acellular, and the cell population that forms it is not known.

We therefore wanted to locate the TCF + cells with respect to other barbel structures, particularly the central rod and the epidermal-dermal boundary. To obtain maximum resolution for these studies, we performed transmission electron microscopy on cross-sections of adult barbel tissue.

Within these sections, we attempted to identify the TCF+ population based on our prior observation of the sub-epithelial, circumferential arrangement and strongly flattened nuclear morphology of these cells. In each highly magnified maxillary barbel cross-section, we observed a ring of cells with these features. Assuming that these are the same cells identified by the TCF siam:mCherry nuclear label, we will refer to them as the ‘TCF+ cells.’ In the following description we review the structural features of the maxillary barbel and the histological context of this novel cell type. The ZMB in cross-section presents a dermal core of cells and matrix surrounded by a multilayered epithelium. The epithelial layer features an electron-dense cytoplasm and abundant tight junctions between adjacent cells.

These cells rest on a prominent basement membrane with a thick collagen underlayer. This membrane defines the epidermal-dermal boundary. The TCF+ cells occupy the subadjacent dermal compartment and are easily identified by their large, flat nuclei. Surrounding each nucleus are ribbons of convoluted cytoplasm in close contact with surrounding collagen bundles.

Notably, each of the TCF+ cells is entirely embedded within the matrix of the central rod, approximately 2–3 microns below the rod surface. Transmission electron microcopy of the TCF+ ZMB core cells In sections not intersecting TCF+ cell nuclei, we observed a circumferential ring of matrix-bound cytoplasm at a similar depth. Within this ring, membrane-localized tight junctions indicate overlapping cytoplasmic projections from multiple cells.

Although most of these projections were circumferential, there are occasional radial or oblique extensions. These blunt or tapered arms extend up to one micron into the surrounding matrix. Within each TCF+ cell we observed a dense granular cytoplasm enriched with rough endoplasmic reticulum. Finally, deep to the TCF+ cells lies a broad region of acellular collagenous matrix, representing the remainder of the barbel core. Interestingly, the matrix immediately adjacent to the TCF+ cells appeared more electrolucent, in contrast to this central region, which was more electron-dense. Collagen bundles near the TCF+ cells appeared loosely packed, with well-separated circular cross-sections through individual triple helices.

In contrast, the matrix distant from the cells appeared more homogeneous with few or no inter-fibrillar gaps. This may indicate hyperpolymerization of collagen towards the more central regions of the appendage. Evolution and morphogenesis of skin appendages In this study we provide several new observations on the development of barbels, a widely distributed structure in amphibians, reptiles, and fishes (;; ). Urodele tadpoles, for example, have a pair of rod-like structures, known as balancers, which develop in the branchial region and are used to attach to underwater substrates.

Erpeton tentaculus, an aquatic snake, has a pair of highly innervated cranial tentacles that sense prey (; ). Barbel-like appendages are also common in teleost fishes, with almost half of the existing orders having one or more barbelled species. Such barbels can be paired or unpaired, can extend from different regions of the head or body, and can be sexually dimorphic. Within the Cyprinidae, the clade to which zebrafish belong, some species have paired barbels and others lack them. These appendages are thought to have evolved repeatedly, representing either independent adaptations, or convergent regressions to an ancestral condition. Although variability in barbel number, position, and function is well documented, there are few studies on the ontogenetic mechanisms by which these structures emerge.

An understanding of how barbels originate at the cellular and molecular levels, using zebrafish as a model, may help to explain the diversity of barbel distribution and composition within cyprinids as a whole. Comparative developmental studies of other barbelled fishes, including both laboratory- and commercially-reared fish species, may illuminate more generally the mechanisms by which barbels have evolved repeatedly in many lineages of fish phylogeny. Changes in cell shape and distribution Local and regional cell-shape changes are often critical first steps in the organization of appendages.

The classic discovery of epithelial-mesenchymal organizing centers, such as the apical ectoderm ridge, or AER, strongly inform research and reviews of appendage outgrowth. A similar mechanism has been observed during zebrafish fin development, in which an apical ectodermal ridge becomes an apical fold (AF), an organizing structure in the fin bud. Removal of the chick AER causes limb truncations , whereas removal of the zebrafish AF causes mesenchymal elongation. These and other experiments have shown that epithelial ridges and folds are key molecular centers for appendage development, and that ectopic expression, genetic mutation, or chemical disruption can strongly affect the morphological result.

Most broadly, the reciprocal interactions at these influential sites are thought to represent ancestral genetic “cassettes” or regulatory “modules” that have been used repeatedly in vertebrate phylogeny. It is important to note, however, that alternative methods of appendage development may occur, particularly in structures not homologous to limbs. In this study, we observed that the first morphological sign of maxillary barbel outgrowth is a mesenchymal condensation within the dermis of the maxilla. However, there is no corresponding epidermal structure, such as a placode or AER.

Rather, the distal epithelial cells of the barbel remain rounded or become progressively flattened as the appendage grows. Outgrowth of the ZMB thus differs from vertebrate limb development, but appears morphologically similar to the barbels of the channel catfish or the balancers of urodele tadpoles. These latter structures have a rounded epithelial cover at the slightly bulbous or cone-shaped distal end, but no particular ridge or other apical structure.

Vwr 1530 Incubator Manual

How, then, do these structures receive the signal to grow? Lacking an AER, these appendages may receive local genetic signals that are functionally equivalent. Gene expression studies in catfish barbels, for example, demonstrate that transcripts for FGFs, Shh, Dlx and other key ligands can be spatially restricted even within the continuous epithelium of the developing appendage. Therefore one or more signaling molecules may yet be discovered that instruct the areas from which zebrafish barbels eventually grow. Patterns of cell proliferation Appendages reach their final shape and size through coordinated cell division, cell migration, and cell death. Of these, we examined the cell division patterns in the maxillary barbel to determine whether they were concentrated proximally or distally, restricted to a “progress zone”, or randomly arranged. Similar techniques have been used on other developing zebrafish structures, leading to more precise models of their growth mechanics.

Using 5′-bromo-2′-deoxyuridine (BrdU) to label dividing cells during juvenile caudal fin developmentshowed that cells in the dorsal and ventral fin rays proliferate faster than cells in the central fin rays. This different in rate causes the blunt-ended larval structure to grow into the characteristic bi-lobed shape of the adult. More recently, in vivo EdU labeling was used to locate mitotic cells in the embryonic zebrafish notochord, which are concentrated at the distal end. Mapping local patterns of cell division can thus identify highly mitotic precursors that contribute maximally to appendage outgrowth.

In this report, we used an in vitro explant culture system to label patterns of cell proliferation in the developing ZMB. In contrast to the zebrafish caudal fin and notochord, in which there is a strong positional gradient of cells in S-phase, there is no similar pattern in the maxillary barbel. Over a tenfold increase in barbel length– from 100 microns to 1 mm– labeled nuclei appeared evenly distributed in proximal and distal areas of this appendage.

Most of these cell divisions were in the basal layer of the epithelium, as expected for a healthy layer of skin. Occasional divisions were detected in deeper cells, including the novel “core cells” described here. However, these were not localized along any appendage axis. This suggests that the developing maxillary barbel has a “pan-appendage” growth pattern. An alternative method of EdU labeling in zebrafish is peritoneal injection of the compound.

However, this requires more expertise in animal handling, two handling procedures per fish (once at administration and once at collection) and more EdU per fish to label all body tissues, not all of which are collected or used. In our short-term plate-based assay, we achieved good EdU labeling of small, whole tissue fragments using minimal reagent, while exposing each fragment to the same concentration of label.

Vwr Incubator Model 2325 Manual Transmission Diagram

Tissue integrity was maintained well, and all fragments yielded good quality nuclear staining. Although the long-term physiology of explanted tissues may not be identical to the corresponding tissues in vivo, the short-term capacity to see and manipulate cellular processes is enhanced. Historically, L-15 explant culture has been used to maintain fragments of fish and amphibian tissues– including gonad , thyroid , pancreas , and gill – for periods of days to weeks. Similar techniques may be of interest to researchers wishing to simultaneously label and/or visualize cellular events in a convenient plate-based format. Fishing for Wnts; identification of a novel, TCF+ mesenchymal cell population in maxillary barbel development All appendages arise from interactions between two adjacent layers: an outer epithelium and an inner mesenchyme.

A key evolutionary question, then, is how the same two layers interact to produce diverse skin appendages in different animal species. Embryologically, the trunk and tail dermis comes from the dermatomal layer of the somite , whereas the head dermis, which forms anterior appendages such as barbels, comes from cranial neural crest cells. In general, the dermis directs the size, shape, and distribution of skin appendages by exchanging signals with the epidermis. Highly conserved molecular pathways such as wingless (Wnt), fibroblast growth factor (FGF), bone morphogenetic protein (BMP), and Hedgehog (Hh) mediate these dermal-epidermal interactions and are essential for the proper formation of mammalian hairs (; ), avian feathers , and reptilian scales (Chang et al.

Therefore, it is thought that variations in the timing and expression of these signals produce an “appendage spectrum” of novelty and diversity across animal taxa. The transparent ZMB is an ideal context in which to observe the genetic signaling of these adjacent cell layers, using the optical tools of the zebrafish model. In this study, we used the TCF siam transgenic zebrafish line, which was designed to provide a visible readout of the canonical Wnt pathway. Specifically, this line displays intense nuclear mCherry expression in cells expressing TCF, a DNA-binding component of canonical Wnt signaling. Our analysis of this line indicates a strong TCF+ cell population within early-budding, elongating and adult barbel tissue. Co-localization of the reporter-labeled nuclei with EdU labeling shows that the TCF+ cells are occasionally mitotic, but not highly proliferative relative to surrounding cells. Using TEM, we further located the TCF+ cells to a single, circumferential layer underneath the basement membrane and within the dermal core.

Similar to osteoblasts, these barbel “core cells” are entirely encased in surrounding matrix, but connect to each other via small cytoplasmic projections. In addition to their unique location, cells within this layer are identified by their pancake-shaped nuclei and abundant RER. How to build a barbel: ultimate and proximate mechanisms The ultimate mechanism of barbel development may be the global metamorphic transformation of the larval zebrafish to a juvenile, a process occurring 3–4 weeks post-fertilization , This period includes multiple morphological and physiological changes, including alterations in fin morphology, external pigmentation, and circulating hormone levels. Considering the proximate mechanisms for barbel outgrowth, the TCF+ cells within this appendage likely play a key role. Specifically, we speculate that their function is not to divide, but to produce collagenous matrix in response to Wnt signals, which are present in a proximal-distal gradient along the appendage. There are two possibilities for the source of the putative Wnt ligand. In a paracrine mechanism, the source is the adjacent epithelium (, top).

In this model, sufficient ligand must pass through the basement membrane and subadjacent collagenous layers for the matrix-bound mesenchymal cells to detect it, possibly via their short cytoplasmic projections. In an autocrine mechanism (, bottom), the TCF+ cells are themselves the ligand source, cooperatively maintaining a Wnt-enriched environment. In conclusion, we propose a model of barbel outgrowth consistent with our collective observations. In response to unspecified proximal signals from the epidermis, a pre-barbel condensation forms within the dermis lateral to the maxillary bone. Cells within this whorl divide, extending a dermal bud. Specific cells within this bud become entrained in a Wnt-responsive signal loop, and begin to secrete the collagenous matrix that will form the barbel core. The secretory subpopulation forms a radially flattened, circumferentially arranged “growth ring”, which can gradually add to barbel length and girth throughout the lifespan.

Cells within the ring contact each other through cytoplasmic bridges, and divide only when needed to maintain a single-cell layer. As the barbel matures, the matrix-producing cells at the proximal end decrease or halt decreasing matrix production.

Vwr Incubator Model 2325 Manual Transmission Fluid

Cells at the tip, however, maintain Wnt-responsiveness, constantly contributing to the most recently assembled part of the appendage. Although much of this model remains unexplored, similar gene, expression, cell behavior and matrix mechanics may be responsible for the independent and repeated evolution of barbel structures in other fish species. Research funding was provided by NIH R15-HD064169 (to E.E.L.).

A portion of this work was performed in partial fulfillment of the academic requirements for the Master of Science at DePaul University (S.S.). Confocal reconstruction was made possible in part by FluoRender software from the University of Utah, funded by NIH R01-GM098151-01. Transmission electron microscopy was performed at the Northwestern University Center for Advanced Microscopy, which is generously supported by NCI CCSG P30 CA060553, awarded to the Robert H.

Lurie Comprehensive Cancer Center. Lennell Reynolds provided expert TEM specimen preparation.

We thank Jacek Topczewski and two anonymous reviewers for critical comments on the manuscript.