We thank Dr. Steven Austad for providing us with the first version of this protocol. This work was supported by grants from the NIH and the Ellison Medical Foundation to V.G. and A.S.

1. Before Starting
<ol>
 <li> Sterilize scissors and forceps with 70% ethanol.</li>
 <li> Place small magnetic stirrer inside a 30 mL beaker, cover with two layers of foil, and autoclave.</li>
 <li> Prepare a 28 Wunsch units/mL stock solution of Liberase Blendzyme 3 in sterile water. Make 0.5 mL aliquots and freeze at -20&deg;C. Thaw a new aliquot before every use. The solution may appear cloudy after thawing. Vortex the solution until it becomes clear.</li>
 <li> Warm up the cell culture media.</li>
</ol>
2. Animal Sample Preparation
Caution: wild animals may contain pathogens such as a rabies virus. Always be aware of open sharps.
<ol>
 <li> Euthanize the animal and place the carcass at 4&deg;C. It is best to use the carcass immediately, however, if this is not practical such as if the animals are collected in the field, the carcasses may be used within 24 hours. After 24 hours the cell yield declines.</li>
 <li> Dissect the animal in the surgical suite or in chemical hood (not in tissue culture hood).</li>
 <li> Underarm area is a convenient site to collect skin samples as underarm skin is thinner, contains less fat, and the fur is less dense. Clean the incision site with 70% ethanol. Make sure the fur is soaked with ethanol. </li>
 <li> Shave the fur around the incision site with a sharp scalpel. Shave a larger area than the desired incision site. Try to minimize cuts to the skin. Spray the area with 70% ethanol and let it dry.</li>
 <li> To collect a skin sample excise a fragment of approximately 1 cm2. Pinch the skin with tissue forceps, and cut with scissors. Try not to cut the fat layer with the skin, as fat interferes with collagenase digestion. To collect the lung samples, wash the chest area with 70% ethanol, and open the skin on the chest with scissors by making a T-shape incision and pulling apart the flaps of the skin. Wash the opened muscle area with 70% ethanol and let dry. Cut the rib cage using sterile forceps and scissors (use bone cutters for larger animals). Use sterile techniques to avoid contaminating internal organs. Do not touch the internal organs with instruments that touched the animal fur. Cut lung fragments of approximately 1 cm2 using sterile forceps and scissors.</li>
 <li> Place tissue fragments in 50 mL tubes with sterile PBS to avoid drying.</li>
 <li> Wash the outside of the 50 mL tubes with tissue fragments with ethanol, and take them to the tissue culture hood.</li>
 <li> Properly dispose of animal carcass.</li>
</ol>
3. Extracting Cells
<ol>
 <li> Transfer the tissue fragments into a 10 cm tissue culture dish using sterile scalpel. Do not transfer too much PBS with the sample.</li>
 <li> Cut the tissue into ~1 mm pieces using two scalpels. Use two blades using a scissor action starting from the center and pulling apart. Keep the tissue balled up, do not cut piece by piece. When the cutting is sufficient the skin resembles putty, it will not separate into pieces but will stretch thin. The lung tissue is easier to cut, and it will separate into tiny pieces.</li>
 <li> Using a scalpel, transfer the cut tissue into sterile 30 mL beaker with sterile stir bar. Wash the plate used for cutting tissue with 10 mL of DMEM/F12 media with 0.14 Wunsch units/mL Liberase Blendzyme 3, and 1X antibiotic/antimycotic, and add the solution to the 30 mL beaker with tissue fragments.</li>
 <li> Cover the beaker with sterile foil, and incubate at 37&deg;C, stirring slowly, for 30 to 90 minutes. The length of the incubation depends on the species and tissue type. Take care not to over-digest the tissue. Best yields are obtained when tissue fragments are still present at the end of the digestion. Skin takes longer to digest than the lung. Skin from large animals takes longer to digest. Check the digestion after 30 min, and then every 10 min. When the skin digestion is complete, the media becomes cloudy and skin fragments separate from each other, and the edges of the pieces become "fuzzy". Lung digestion should be stopped when lung fragments change color from red to white and start forming sticky fibers.</li>
 <li> Pipet the solution containing tissue fragments up and down to break the clumps. Transfer the solution to sterile 50 mL tube. If the fragments move easily through the 10 mL pipette cutting and digestion was done well. Rinse the beaker 3 times with 10 mL of warm DMEM/F12 media with 15% FBS, 1X antibiotic/antimycotic and add the media to the 50 mL tube with tissue fragments. Close the 50 mL tube and mix by inversion a few times. The FBS in the media will stop Liberase digestion.</li>
 <li> Spin at 524 g in a swinging bucket tissue culture centrifuge for 5 min. Remove the supernatant. Resuspend the pellet in 10 mL of warm DMEM/F12 media with 15% FBS, 1X antibiotic/antimycotic. Pipet the suspension with maximum force to break the tissue pieces.</li>
 <li> Add another 30 mL of DMEM/F12 media with 15% FBS, 1X antibiotic/antimycotic, mix and centrifuge at 524 g in a swinging bucket tissue culture centrifuge for 5 min. Repeat one more time to remove the traces of Liberase.</li>
 <li> Resuspend the pellet in 10 mL of DMEM/F12 media with 15% FBS, 1X antibiotic/antimycotic and transfer to a 10 cm tissue culture dish and place in a tissue culture incubator at 37&deg;C, 5%CO2, 3%O2.</li>
 <li> Check the plates every day for fibroblasts and media color. If the isolation was successful, fibroblasts crawl out of the tissue fragments and attach to the plate (Figure 1). The fibroblast start to exit tissue fragments within 2-5 days.</li>
 <li> If the media changes color to yellow, this indicates potential contamination or overcrowding of cells. Examine the plates under the microscope at high magnification. If bacteria, fungi, or worms are present discard the plates (this is rarely an issue with laboratory animals, however may occur when the samples are collected from the wild). If no contamination is present, but the media changed color, this is caused by either too many cells or too many tissue fragments placed in the same dish. If more than 60% of the plate is covered by attached fibroblasts, change the media on the plate and transfer the tissue fragments to a new plate with the new media. If not many fibroblasts attached to the plate, change the media and split the tissue pieces to a 2-4 plates.</li>
 <li> After 7 days, if media had not been changed earlier, change the media and transfer the tissue fragments to a new plate with new media. </li>
 <li> Incubate the cells and tissue fragments for an additional 7 days. By day 14 all viable fibroblasts have exited the tissue fragments.</li>
 <li> After 14 days from the beginning of the cell isolation, discard the old media and tissue fragments, harvest the cells and plate them on a new plate at 5x105 cells/plate EMEM with 15% FBS, 1X Penicillin/Streptomycin, non essential amino acids, and sodium pyruvate. EMEM media will support growth of fibroblasts only and other cell types will die or stop proliferating.</li>
 <li> After the cells reach 80-90% confluence, freeze an aliquot of cells for future use.</li>
 <li> Continue culturing the cells by splitting them at 5x105 cells/plate when the cells reach 80-90% confluence.</li>
</ol>
4. Representative Results
Normal fibroblasts are large cells with prominent protrusions (lamellipodia) (Figure 2). Fibroblasts grow in a monolayer. A healthy growing culture contains 1-10% cells in M stage, recognized as rounded up cells elevated over the surface of the plate, but not detached from the plate (Figure 3). Typically, a 10 cm dish seeded with 5x105 cells becomes confluent in 3-4 days. The doubling time varies greatly between species, and may be greater for some of the long-lived rodent species1. When cells fill a plate they arrest proliferation in G1 stage. Typical confluent plate of fibroblasts contains a tightly packed layer of cells (Figure 4). When the cells reach 90% confluence they are ready for splitting. If desired, the cells can be maintained on an arrested confluent plate for extended periods of time with regular media changes (once or twice a week).
<img src="/files/ftp_upload/2033/2033fig1.jpg" alt="Figure 1" /> 
Figure 1. Fibroblast isolation from mouse skin (A) and lung (B). The media was changed to remove unattached cells and debris prior to taking the pictures on Day 7.
<img src="/files/ftp_upload/2033/2033fig2.jpg" alt="Figure 2" /> 
Figure 2. Mouse lung fibroblasts. 
<img src="/files/ftp_upload/2033/2033fig3.jpg" alt="Figure 3" /> 
Figure 3. A field of mouse fibroblasts containing cells in M-stage, photographed at 10X magnification. 
<img src="/files/ftp_upload/2033/2033fig4.jpg" alt="Figure 4" /> 
Figure 4. A confluent plate of mouse fibroblasts, photographed at 10X magnification.

<ol>
	<li>Seluanov, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Distinct+tumor+suppressor+mechanisms+evolve+in+rodent+species+that+differ+in+size+and+lifespan.+Aging+.">Distinct tumor suppressor mechanisms evolve in rodent species that differ in size and lifespan. Aging .</a> Cell. 7, 813-823 (2008).</li><li>Parrinello, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Oxygen+sensitivity+severely+limits+the+replicative+lifespan+of+murine+fibroblasts.">Oxygen sensitivity severely limits the replicative lifespan of murine fibroblasts.</a> Nat Cell Biol. 5, 741-747 (2003).</li></ol>

No conflicts of interest declared.

Normal primary fibroblasts provide an excellent alternative to established cancer cell lines in biological research. An important advantage of fibroblasts is that they do not carry mutations in oncogenes and tumor suppressors and maintain intact cell cycle checkpoints. This makes normal fibroblasts a preferred system for the studies of cell cycle regulation, DNA repair, and apoptosis. The protocol described here provides a simple recipe for isolation and maintenance of primary fibroblasts. This protocol was used to succe...

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<html xmlns="http://www.w3.org/1999/xhtml" xml:lang="en" lang="en">	
		
		<div>
		<table border="1">
		<thead>
		<tr>
		<th>Material Name</th>
		<th>Type</th>
		<th>Company</th>
		<th>Catalogue Number</th>
		<th>Comment</th>
		</tr>
		</thead>
		<tbody>
		
<tr>
<td>DMEM/F12 media</td>
<td>&nbsp;</td>
<td>Invitrogen</td>
<td>11330-032</td>
<td>&nbsp;</td>
<tr>
<td>Fetal Bovine Serum (FBS), Qualified</td>
<td>&nbsp;</td>
<td>Invitrogen</td>
<td>01437-036</td>
<td>The Qualified serum had been pre-tested to provide good growth support for primary fibroblasts.</td>
</tr>
<tr>
<td>Antibiotic/Antimycotic</td>
<td>&nbsp;</td>
<td>Invitrogen</td>
<td>15420-096</td>
<td>&nbsp;</td>
<tr>
<td>Penicillin/Streptomycin</td>
<td>&nbsp;</td>
<td>Invitrogen</td>
<td>15140-122</td>
<td>&nbsp;</td>
<tr>
<td>Liberase TM Research Grade</td>
<td>&nbsp;</td>
<td>Roche</td>
<td>05401127001</td>
<td>Replacement enzyme.</td>
<tr>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>A note from the authors:
Since Roche discontinued Liberase Blendzyme 3 (11814184001), they recommend using Liberase TM Research Grade medium Thermolysin (Cat. no. 05401119001 - 10 mg, Cat. no. 05401127001 - 100mg) instead. We have switched to this enzyme successfully with no issues.</td>
<tr>
<td>EMEM media</td>
<td>&nbsp;</td>
<td>ATCC</td>
<td>30-203</td>
<td>The EMEM media from ATCC already contains nonessential amino acids and sodium pyruvate.</td>
</tr>
<tr>
<td>Feathered #21 disposable, sterile scalpel</td>
<td>&nbsp;</td>
<td>Multiple suppliers</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<tr>
<td>Three Gas Control incubator</td>
<td>&nbsp;</td>
<td>Forma or Heraeus</td>
<td>&nbsp;</td>
<td>&nbsp;</td>		</tbody>
		</table>
		</div>

establishing primary adult fibroblast cultures from rodents

The importance of using primary cells, rather than cancer cell lines, for biological studies is becoming widely recognized. Primary cells are preferred in studies of cell cycle control, apoptosis, and DNA repair, as cancer cells carry mutations in genes involved in these processes. Primary cells cannot be cultured indefinitely due to the onset of replicative senescence or aneuploidization. Hence, new cultures need to be established regularly. The procedure for isolation of rodent embryonic fibroblasts is well established, but isolating adult fibroblast cultures often presents a challenge. Adult rodent fibroblasts isolated from mouse models of human disease may be a preferred control when comparing them to fibroblasts from human patients. Furthermore, adult fibroblasts are the only available material when working with wild rodents where pregnant females cannot be easily obtained. Here we provide a protocol for isolation and culture of adult fibroblasts from rodent skin and lungs. We used this procedure successfully to isolate fibroblasts from over twenty rodent species from laboratory mice and rats to wild rodents such as beaver, porcupine, and squirrel.

Watch this Scientific Journal Video about Establishing Primary Adult Fibroblast Cultures From Rodents at JoVE.com

Establishing Primary Adult Fibroblast Cultures From Rodents

This article describes a protocol for isolation and maintenance of primary fibroblast cultures from skin and lung tissue of wild rodents.

The importance of using primary cells, rather than cancer cell lines, for biological studies is becoming widely recognized.  Primary cells are preferred ...

establishing-primary-adult-fibroblast-cultures-from-rodents

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49.2K 조회수.  University of Rochester. 이 문서는 고립과 야생 설치류 동물의 피부와 폐 조직에서 기본 fibroblast 문화의 유지 관리를위한 프로토콜을 설명합니다.

비디오: Establishing Primary Adult Fibroblast Cultures From Rodents

Primary Neuronal Cultures from the Brains of Late Stage Drosophila Pupae

In this video, we demonstrate the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. The procedure begins with the removal of brains from animals at 70-78 hrs after puparium formation. The isolated brains are shown after brief incubation in papain followed by several washes in serum-free growth medium. The process of mechanical dissociation of each brain in a 5 ul drop of media on a coverslip is illustrated. The axons and dendrites of the post-mitotic neurons are sheered off near the soma during dissociation but the neurons begin to regenerate processes within a few hours of plating. Images show live cultures at 2 days. Neurons continue to elaborate processes during the first week in culture. Specific neuronal populations can be identified in culture using GAL4 lines to drive tissue specific expression of fluorescent markers such as  GFP or RFP. Whole cell recordings have demonstrated the cultured neurons form functional, spontaneously active cholinergic and GABAergic synapses. A short video segment illustrates calcium dynamics in the cultured neurons using Fura-2 as a calcium indicator dye to monitor spontaneous calcium transients and nicotine evoked calcium responses in a dish of cultured neurons. These pupal brain cultures are a useful model system in which genetic and pharmacological tools can be used to identify intrinsic and extrinsic factors that influence formation and function of central synapses.

This video demonstrates the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. Views of live cultures show neurite outgrowth and imaging of calcium levels using Fura-2.

In this video, we demonstrate the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. The procedure begins with the ...

Primary Dissociated Midbrain Dopamine Cell Cultures from Rodent Neonates

The ability to create primary cell cultures of dopamine neurons allows for the study of the presynaptic characteristics of dopamine neurons in isolation from systemic input from elsewhere in the brain. In our lab, we use these neurons to assess dopamine release kinetics using carbon fiber amperometry, as well as expression levels of dopamine related genes and proteins using quantitative PCR and immunocytochemistry. In this video, we show you how we generate these cultures from rodent neonates.
The process involves several steps, including the plating of cortical glial astrocytes, the conditioning of neuronal cell culture media by the glial substrate, the dissection of the midbrain in neonates, the digestion, extraction and plating of dopamine neurons and the addition of neurotrophic factors to ensure cell survival.
The applications suitable for such a preparation include electrophysiology, immunocytochemistry, quantitative PCR, video microscopy (i.e., of real-time vesicular fusion with the plasma membrane), cell viability assays and other toxicological screens.

Primary dissociated midbrain dopamine cell cultures allow for the study of presynaptic characteristics of dopamine neurons. They can be used to monitor real-time dopamine release kinetics and protein/mRNA levels of regulators of dopamine exocytosis. Here, we show you how to generate these cultures from rodent neonates.

The ability to create primary cell cultures of dopamine neurons allows for the study of the presynaptic characteristics of dopamine neurons in isolation ...

The Preparation of Primary Hematopoietic Cell Cultures From Murine Bone Marrow for Electroporation

It is becoming increasingly apparent that electroporation is the most effective way to introduce plasmid DNA or siRNA into primary cells. The Gene Pulser MXcell  electroporation system and Gene Pulser  electroporation buffer were specifically developed to transfect nucleic acids into mammalian cells and difficult-to-transfect cells, such as primary and stem cells.This video demonstrates how to establish primary hematopoietic cell cultures from murine bone marrow, and then prepare them for electroporation in the MXcell system. We begin by isolating femur and tibia. Bone marrow from both femur and tibia are then harvested and cultures are established. Cultured bone marrow cells are then transfected and analyzed.

This procedure describes how to establish primary hematopoietic cell cultures from murine bone marrow and is followed by transfection using the Gene Pulser MXCell electroporation system.

It is becoming increasingly apparent that electroporation is the most effective way to introduce plasmid DNA or siRNA into primary cells. The Gene Pulser ...

Primary Culture of Adult Rat Heart Myocytes

Cultured primary adult rodent heart cells are an important model system for cardiovascular research. Nevertheless, establishment of robust, viable cultured adult myocytes can be a technically challenging, rate-limiting step for many researchers. Here we described a protocol to obtain a high yield of adult rat heart myocytes that remain viable in culture for several days. The heart is isolated and perfused with collagenase and protease under low Ca2+ conditions to recover single myocytes. Ca2+-tolerant cells are obtained by stepwise increases in extracellular Ca2+ concentration in three subsequent wash steps. Cells are filtered, resuspended in culture medium, and plated on laminin coated slips. Cultured myocytes obtained using this protocol are viable for up to four days and are suitable for most experiments including electrophysiology, biochemistry, imaging and molecular biology.

In this paper, we described a typical way to isolate and culture adult rat heart myocytes. Collagenase and protease are used to digest and isolate single myocytes. Myocytes cultured follow this protocol meet most experiment requirements.

Cultured primary adult rodent heart cells are an important model system for cardiovascular research.  Nevertheless, establishment of robust, viable ...

Primary Cell Cultures from Drosophila Gastrula Embryos

Here we describe a method for preparing and culturing primary cells dissociated from Drosophila gastrula embryos. In brief, a large amount of staged embryos from young and healthy flies are collected, sterilized, and then physically dissociated into a single cell suspension using a glass homogenizer. After being plated on culture plates or chamber slides at an appropriate density in culture medium, these cells can further differentiate into several morphologically-distinct cell types, which can be identified by their specific cell markers. Furthermore, we present conditions for treating these cells with double stranded (ds) RNAs to elicit gene knockdown. Efficient RNAi in Drosophila primary cells is accomplished by simply bathing the cells in dsRNA-containing culture medium. The ability to carry out effective RNAi perturbation, together with other molecular, biochemical, cell imaging analyses, will allow a variety of questions to be answered in Drosophila primary cells, especially those related to differentiated muscle and neuronal cells.

Primary Cell Cultures from Drosophila Gastrula Embryos

We provide a detailed protocol for preparing primary cells dissociated from Drosophila embryos. The ability to carry out the effective RNAi perturbation, together with other molecular, biochemical and cell imaging methods will allow a variety of questions to be addressed in Drosophila primary cells.

Here we describe a method for preparing and culturing primary cells dissociated from Drosophila gastrula embryos.   In brief, a large amount of staged ...

Rapid Fibroblast Removal from High Density Human Embryonic Stem Cell Cultures

Mouse embryonic fibroblasts (MEFs) were used to establish human embryonic stem cells (hESCs) cultures after blastocyst isolation1. This feeder system maintains hESCs from undergoing spontaneous differentiation during cell expansion. However, this co-culture method is labor intensive, requires highly trained personnel, and yields low hESC purity4. Many laboratories have attempted to minimize the number of feeder cells in hESC cultures (i.e. incorporating matrix-coated dishes or other feeder cell types5-8). These modified culture systems have shown some promise, but have not supplanted the standard method for culturing hESCs with mitomycin C-treated mouse embyronic fibroblasts in order to retard unwanted spontaneous differentiation of the hESC cultures. Therefore, the feeder cells used in hESC expansion should be removed during differentiation experiments. Although several techniques are available for purifying the hESC colonies (FACS, MACS, or use of drug resistant vectors) from feeders, these techniques are labor intensive, costly and/or destructive to the hESC. The aim of this project was to invent a method of purification that enables the harvesting of a purer population of hESCs. We have observed that in a confluent hESC culture, the MEF population can be removed using a simple and rapid aspiration of the MEF sheet. This removal is dependent on several factors, including lateral cell-to-cell binding of MEFs that have a lower binding affinity to the styrene culture dish, and the ability of the stem cell colonies to push the fibroblasts outward during the generation of their own "niche". The hESC were then examined for SSEA-4, Oct3/4 and Tra 1-81 expression up to 10 days after MEF removal to ensure maintenance of pluripotency. Moreover, hESC colonies were able to continue growing from into larger formations after MEF removal, providing an additional level of hESC expansion.

Despite ongoing efforts to transition cultures to feeder-free conditions, the derivation and culture of human embryonic stem cells (hESC) remain largely dependent on co-cultures with mouse embryonic feeders (MEFs). Here, we show a novel methodology for rapidly removing feeders from hESC cultures prior to experimentation.

Mouse embryonic fibroblasts (MEFs) were used to establish human embryonic stem cells (hESCs) cultures after blastocyst isolation1. This feeder system ...

Na&iuml;ve Adult Stem Cells Isolation from Primary Human Fibroblast Cultures

Over the last decade, several adult stem cell populations have been identified in human skin 1-4. The isolation of multipotent adult dermal precursors was first reported by Miller F. D laboratory 5, 6. These early studies described a multipotent precursor cell population from adult mammalian dermis 5. These cells--termed SKPs, for skin-derived precursors-- were isolated and expanded from rodent and human skin and differentiated into both neural and mesodermal progeny, including cell types never found in skin, such as neurons 5. Immunocytochemical studies on cultured SKPs revealed that cells expressed vimentin and nestin, an intermediate filament protein expressed in neural and skeletal muscle precursors, in addition to fibronectin and multipotent stem cell markers 6. Until now, the adult stem cells population SKPs have been isolated from freshly collected mammalian skin biopsies.
Recently, we have established and reported that a population of skin derived precursor cells could remain present in primary fibroblast cultures established from skin biopsies 7. The assumption that a few somatic stem cells might reside in primary fibroblast cultures at early population doublings was based upon the following observations: (1) SKPs and primary fibroblast cultures are derived from the dermis, and therefore a small number of SKP cells could remain present in primary dermal fibroblast cultures and (2) primary fibroblast cultures grown from frozen aliquots that have been subjected to unfavorable temperature during storage or transfer contained a small number of cells that remained viable 7. These rare cells were able to expand and could be passaged several times. This observation suggested that a small number of cells with high proliferation potency and resistance to stress were present in human fibroblast cultures 7.
We took advantage of these findings to establish a protocol for rapid isolation of adult stem cells from primary fibroblast cultures that are readily available from tissue banks around the world (Figure 1). This method has important significance as it allows the isolation of precursor cells when skin samples are not accessible while fibroblast cultures may be available from tissue banks, thus, opening new opportunities to dissect the molecular mechanisms underlying rare genetic diseases as well as modeling diseases in a dish.

Na&amp;#239;ve Adult Stem Cells Isolation from Primary Human Fibroblast Cultures

We report a method to isolate na&#239;ve multipotent skin-derived precursor (SKP) cells from primary human fibroblast cultures. We show that these SKPs derived from fibroblast cultures share similar stem cell properties to the ones derived directly from human skin biopsies. These cells express the neural crest marker, nestin, in addition to the multipotent markers such as OCT4 and Nanog.

Over the last decade, several adult stem cell  populations have been identified in human skin 1-4.  The isolation of multipotent adult dermal precursors ...

Preparation of Primary Myogenic Precursor Cell/Myoblast Cultures from Basal Vertebrate Lineages

Due to the inherent difficulty and time involved with studying the myogenic program in vivo, primary culture systems derived from the resident adult stem cells of skeletal muscle, the myogenic precursor cells (MPCs), have proven indispensible to our understanding of mammalian skeletal muscle development and growth. Particularly among the basal taxa of Vertebrata, however, data are limited describing the molecular mechanisms controlling the self-renewal, proliferation, and differentiation of MPCs. Of particular interest are potential mechanisms that underlie the ability of basal vertebrates to undergo considerable postlarval skeletal myofiber hyperplasia (i.e.&#160;teleost fish) and full regeneration following appendage loss (i.e.&#160;urodele amphibians). Additionally, the use of cultured myoblasts could aid in the understanding of regeneration and the recapitulation of the myogenic program and the differences between them. To this end, we describe in detail a robust and efficient protocol (and variations therein) for isolating and maintaining MPCs and their progeny, myoblasts and immature myotubes, in cell culture as a platform for understanding the evolution of the myogenic program, beginning with the more basal vertebrates. Capitalizing on the model organism status of the zebrafish (Danio rerio), we report on the application of this protocol to small fishes of the cyprinid clade Danioninae. In tandem, this protocol can be utilized to realize a broader comparative approach by isolating MPCs from the Mexican axolotl (Ambystomamexicanum) and even laboratory rodents. This protocol is now widely used in studying myogenesis in several fish species, including rainbow trout, salmon, and sea bream1-4.

In vitro culture systems have proven indispensible to our understanding of vertebrate myogenesis. However, much remains to be learned about nonmammalian skeletal muscle development and growth, particularly in basal taxa. An efficient and robust protocol for isolating the adult stem cells of this tissue, the myogenic precursor cells (MPCs), and maintaining their self-renewal, proliferation, and differentiation in a primary culture setting allows for the identification of conserved and divergent regulatory mechanisms throughout the vertebrate lineages.

Due to the inherent difficulty and time involved with studying the myogenic program in vivo, primary culture systems derived from the resident adult stem ...

Application of Retinoic Acid to Obtain Osteocytes Cultures from Primary Mouse Osteoblasts

The need for osteocyte cultures is well known to the community of bone researchers; isolation of primary osteocytes is difficult and produces low cell numbers. Therefore, the most widely used cellular system is the osteocyte-like MLO-Y4 cell line.
The method here described refers to the use of retinoic acid to generate a homogeneous population of ramified cells with morphological and molecular osteocyte features.
After isolation of osteoblasts from mouse calvaria, all-trans retinoic acid (ATRA) is added to cell medium, and cell monitoring is conducted daily under an inverted microscope. First morphological changes are detectable after 2 days of treatment and differentiation is generally complete in 5 days, with progressive development of dendrites, loss of the ability to produce extracellular matrix, down-regulation of osteoblast markers and up-regulation of osteocyte-specific molecules.
Daily cell monitoring is needed because of the inherent variability of primary cells, and the protocol can be adapted with minimal variation to cells obtained from different mouse strains and applied to transgenic models. 
The method is easy to perform and does not require special instrumentation, it is highly reproducible, and rapidly generates a mature osteocyte population in complete absence of extracellular matrix, allowing the use of these cells for unlimited biological applications.

Treatment of primary mouse osteoblasts with retinoic acid produces a homogeneous population of ramified cells bearing morphological and molecular features of osteocytes. The method overcomes the difficulty of obtaining and maintaining primary osteocytes in culture, and can be advantageous to study cells derived from transgenic models.&#160;

The need for osteocyte cultures is well known to the community of bone researchers; isolation of primary osteocytes is difficult and produces low cell ...

Isolation and Culture of Primary Mouse Keratinocytes from Neonatal and Adult Mouse Skin

The keratinocyte (KC) is the predominant cell type in the epidermis, the outermost layer of the skin. Epidermal KCs play a critical role in providing skin defense by forming an intact skin barrier against environmental insults, such as UVB irradiation or pathogens, and also by initiating an inflammatory response upon those insults. Here we describe methods to isolate KCs from neonatal mouse skin and from adult mouse tail skin. We also describe culturing conditions using defined growth supplements (dGS) in comparison to chelexed fetal bovine serum (cFBS). Functionally, we show that both neonatal and adult KCs are highly responsive to high calcium-induced terminal differentiation, tight junction formation and stratification. Additionally, cultured adult KCs are susceptible to UVB-triggered cell death and can release large amounts of TNF upon UVB irradiation. Together, the methods described here will be useful to researchers for the setup of in vitro models to study epidermal biology in the neonatal mouse and/or the adult mouse.

Epidermal keratinocytes form a functional skin barrier and are positioned at the front line of host defense against external environmental insults. Here we describe methods for isolation and primary culture of epidermal keratinocytes from neonatal and adult mouse skin, and induction of terminal differentiation and UVB-triggered inflammatory response from keratinocytes.

The keratinocyte (KC) is the predominant cell type in the epidermis, the outermost layer of the skin. Epidermal KCs play a critical role in providing skin ...