This work has been funded by the Hermelin Brain Tumor Center, Henry Ford Hospital.

1. Single Cell Suspension from Fresh Surgical Glioblastoma Specimen for Neurosphere Culture
<ol>
	<li>With written consent from patients and in accordance with institutional guidelines, collect tumor samples for cell culture immediately after resection surgery of high grade glioma.</li>
	<li>Confirm diagnosis of tumor sample by histopathology. Immediately transport the specimen from the operation room to the laminar flow tissue culture hood, for processing within 1 hr from surgery. 
	NOTE: For surgeries at a remote site, cut the tumor sample into smaller fragments and place into a tube containing DMEM/F12 (keep on ice). The tumor can be processed several hours after surgery.</li>
	<li>Starting with 200-500 mg of tissue (optimal), mince the tumor sample using a scalpel blade, and transfer to a 15 ml tube containing 10 ml DMEM/F12 serum-free medium. Mix by inverting several times, let the tumor pieces sediment by gravity, remove medium, and repeat as necessary.</li>
	<li>Prepare the Enzymatic Tissue Dissociation Solution and Stop Solution fresh.
	<ol>
		<li>Enzymatic Tissue Dissociation Solution: 5 ml 0.05% Trypsin-EDTA, 2.5 ml Hank&#8217;s Balanced Salt Solution (HBSS) calcium- and magnesium-free, 2.5 ml Collagenase IV stock solution (2,000 U/ml&#160;in HBSS with calcium and magnesium).</li>
		<li>Stop Solution: 5 ml Trypsin Inhibitor solution, 5 ml DMEM/F12, 2 &#956;l of 5,000 U/ml DNAse I (made in HBSS calcium- and magnesium-free).</li>
	</ol>
	</li>
	<li>Remove medium and add Enzymatic Tissue Dissociation Solution to the minced tumor sample, using 2 ml for each 0.5 g tissue. Gently mix by inverting.</li>
	<li>Incubate the tissue in solution at 37 &#176;C in a tissue culture incubator under rotation for 30 min.</li>
	<li>Triturate with a 2 ml pipette and stop the digestion or return to the incubator for another 15-30 min incubation depending on the level of digestion.</li>
	<li>Stop digestion by adding 2 volumes of Stop Solution and triturate mechanically with a 5 ml serological pipette.</li>
	<li>Filter out the undigested material through a 40 &#956;m cell strainer. Pellet the cells at 800 x g for 5 min at room temp, followed by washing 3x&#160;in 10 ml DMEM/F12.</li>
	<li>Resuspend the final cell pellet in 5 ml DMEM/F12.</li>
	<li>Slowly layer the cell suspension over 5 ml of Lympholyte-M and pellet at 1,300 x g for 20 min at room temperature.</li>
	<li>Transfer the interface layer containing the nucleated cells to a 15 ml tube containing 10 ml of DMEM/F12.</li>
	<li>Pellet the cells at 800 x g for 5 min at room temperature. Repeat the wash with DMEM/F12 2x more.</li>
	<li>Cryopreserve the resulting single cells for further use by resuspending the pellet in Recovery Cell Freezing Medium, aliquoting into cryovials, slow freezing, and storing in liquid nitrogen.</li>
	<li>To culture, resuspend the cells in Neurosphere Medium supplemented with Growth Factors (NMGF), and plate at relatively low density (&#60;1 x 105 cells/ml) in a regular T25 tissue culture flask under standard conditions, 5% CO2, 37 &#176;C, humidified tissue culture incubator (Figure 1A).
	<ol>
		<li>Prepare NMGF using the following recipe
		<table border="0" cellpadding="0" cellspacing="0" width="384">
			<colgroup>
				<col />
				<col />
				<col />
			</colgroup>
			<tbody>
				<tr height="20">
					<td height="20" style="height:20px;width:188px;">For 500 ml of DMEM/F12&#160;</td>
					<td style="width:79px;"></td>
					<td style="width:117px;"></td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">Stock solution</td>
					<td>Volume</td>
					<td>final concentration</td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">N2 supplement (10x)</td>
					<td>5 ml&#160;</td>
					<td>1x</td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">250 mg/ml BSA stock solution&#160;</td>
					<td>1 ml</td>
					<td>0.5 mg/ml</td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">10 mg/ml Gentamicin reagent</td>
					<td>1.25 ml</td>
					<td>25 &#956;g/ml</td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">100x antibiotic/antimycotic</td>
					<td>2.5 ml</td>
					<td>0.5x</td>
				</tr>
				<tr height="20">
					<td>100 mg/ml bFGF</td>
					<td>0.1 ml</td>
					<td>20 ng/ml</td>
				</tr>
				<tr height="20">
					<td height="20" style="height:20px;">100 mg/ml EGF</td>
					<td>0.1 ml</td>
					<td>20 ng/ml</td>
				</tr>
			</tbody>
		</table>
		</li>
	</ol>
	</li>
	<li>Transfer neurospheres that form over 1-3 weeks (Figures 1B-E) to fresh flasks, to separate from attached cells and debris. Perform partial media changes every 3-4 days. 
	NOTE: If dissociating orthotopic xenograft tumor using the protocol above, steps 1.11-1.13 can be omitted.</li>
</ol>
2. Glioblastoma Neurosphere Culture Maintenance and Downstream Applications
<ol>
	<li>Dissociation: Monitor the neurosphere cultures and perform partial medium changes every 3-4 days. When most multicellular neurospheres in the flask reach 100 &#956;m in diameter, dissociate into a single cell suspension:
	<ol>
		<li>Transfer the medium containing the neurospheres to a 15 ml tube, gravity sediment the neurospheres for about 5 min, remove the medium and resuspend the cell pellet in 10 ml calcium- and magnesium-free DPBS.</li>
		<li>Mix and incubate for 10 min at room temperature, as the cells sediment by gravity.</li>
		<li>Remove 7-8 ml of DPBS then dissociate the neurospheres mechanically with a prewetted serological pipette.</li>
		<li>Pellet the dissociated cells at 800 x g for 5 min at 4 &#176;C.</li>
	</ol>
	</li>
	<li>Passaging: Resuspend the dissociated cells (step 2.1.) in NMGF and divide into the necessary number of flasks (1:3), and incubate under standard conditions. Secondary neurospheres will form, and should be subsequently dissociated for the formation of tertiary spheres.</li>
	<li>Assessing long term self-renewal: Repeat the dissociation procedure until the neurosphere culture achieves at least 10 passages, equivalent to a minimum of 2 months in culture.</li>
	<li>Freezing: To cryopreserve the neurospheres, dissociate the neurospheres (step 2.1.) and resuspend the cell pellet in Recovery Cell Freezing Medium, aliquot in cryovials, slow freeze, and store in liquid nitrogen.
	<ol>
		<li>To culture neurosphere cells from a frozen stock: thaw the cells at 37 &#176;C and immediately transfer to a 15 ml tube containing 10 ml DMEM/F12. Mix the tube gently and then spin the cells at 800 x g for 5 min at 4 &#176;C. Wash the cell pellet one more time and resuspend the cells in NMGF and transfer to a T25 tissue culture flask.</li>
	</ol>
	</li>
	<li>Cell suspension for intracranial implant in immunocompromised mouse:
	<ol>
		<li>Dissociate the neurospheres (step&#160;2.1.) and resuspend the cell pellet in calcium- and magnesium-free DPBS. Count viable cells using a hemocytometer and trypan blue exclusion.</li>
		<li>Calculate the number of cells needed for implant, typically 3 x 105 cells/mouse, transfer the desired number of cells into a vial, and pellet the cells at 1,000 x g.</li>
		<li>Resuspend the cell pellet in a volume appropriate for implant (5 &#956;l/mouse) by gently tapping the microcentrifuge tube. Place the cell suspension on ice and use within 2 hr.</li>
	</ol>
	</li>
</ol>
3. Alternative Protocol for Culturing Tumorigenic Glioblastoma Cells (for the cases where neurosphere culture fails)
<ol>
	<li>Supplement the NMGF medium with fetal bovine serum to a final concentration of 2% FBS/NMGF.</li>
	<li>Starting with cells in NMGF culture: Harvest viable cells from the NMGF flask (Figure&#160;1F), resuspend in 2% FBS/NMGF and plate at relatively low density (&#60;1 x 105 cells/ml) in a regular T25 tissue culture flask, and culture under standard conditions, 5% CO2, 37 &#176;C, humidified tissue culture incubator (Figure&#160;1G).</li>
	<li>Starting with frozen never cultured cells (step 1.14.): Thaw the cells, wash in serum-free medium and plate in 2% FBS/NMGF and culture as described in step 3.2. Culturing in NMGF for 3 days prior to transferring viable cells to 2% FBS/NMGF is an alternative to preselect away differentiated cells.</li>
</ol>
4. Morphological and Molecular Analysis of Neurospheres by Immunohistochemistry
<ol>
	<li>Culture the neurospheres until most floating multicellular spheroids reach 100 &#956;m diameter.</li>
	<li>Remove culture flasks from the incubator and immediately pellet the neurospheres, remove medium and add 10 ml of DPBS without disturbing the pellet. Remove DPBS, resuspend in 10% neutral buffered formalin and incubate for 20 min at room temperature.</li>
	<li>Pellet the spheroids, resuspend in 30% ethanol and incubate for 30-45 min.</li>
	<li>Replace 30% ethanol with 50% ethanol, incubate for 15 min and replace with fresh 50% ethanol, incubate a further 30 min.</li>
	<li>Repeat (step 4.4.) with 70% ethanol.</li>
	<li>Replace with 95% ethanol two changes 10-20 min each, and repeat with absolute ethanol until spheroids are bright white and condensed.</li>
	<li>Make a small filter paper cone out of lens paper and place it into a small funnel in a beaker. Wet the lens paper with absolute alcohol.</li>
	<li>Loosen the pellet slightly with fresh 100% ethanol, pour off excess ethanol and pour the spheroids through the lens paper cone, making sure they go to the tip of the cone. Rinse the tube with additional absolute ethanol and pour any remaining spheroids through the lens paper cone.</li>
	<li>Remove the paper cone from the funnel and carefully move the spheroids into the bottom of the cone. Fold the paper into a square and make sure the spheroids are as securely enclosed as possible.</li>
	<li>Transfer the packaged neurospheres to a cassette and transfer to an automatic tissue processor.</li>
	<li>Program the automatic tissue processor as follows: absolute ethanol, 10 min, xylene, 15 min (2x), paraffin, 10 min (4x).</li>
	<li>Remove the cassette from the processor and place it on the heated part of a paraffin embedding system . Make sure the entire surface is free of fragments, dust or other debris and siphon out all paraffin from the forceps warming wells. Warm clean paraffin free forceps and add a small amount of paraffin to a warmed base mold.</li>
	<li>Open the cassette, remove the packet and place it on the heated part of the embedding system. Carefully open the paper cone until the spheroids are visible. Gather as much of the material as possible with prewarmed forceps and transfer to the liquid paraffin in the base mold.</li>
	<li>Repeat as required to retrieve as many of the spheroids as possible. Gently scrape the tissue paper with a prewarmed clean razor blade that has been wiped with ethanol to collect any residual spheroids without getting any paper into the block.</li>
	<li>Carefully break up any spheroid clumps with warm forceps. Move the spheroids away from the corners into a uniform central layer. Move the base mold to the cooling area to secure the spheroids in place, add the cassette, fill slowly with paraffin, and chill thoroughly.</li>
	<li>The neurosphere paraffin block can be used for normal sectioning and immunohistochemistry.</li>
</ol>

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The authors declare that they have no competing financial interests.

Proper enzymatic tumor cell dissociation is a critical step in this protocol. The tissue must be minced well prior to incubation in cell dissociation solution at 37 &#176;C under rotation, for a minimum of 30 min, when the tissue must be mechanically triturated and the extension of the dissociation verified. Depending on the degree of tissue cohesion, incubation can be extended for additional 15-30 min, as needed to complete dissociation into single cells. Incubation in dissociation solution for longer than 1 hr is not recommended due to decreased cell viability. Although the optimal amount of starting tissue is 200-500 mg, this protocol has led to successful neurosphere cultures from as little as 50 mg of tumor tissue.
Serum-free NMGF is a selective medium, and a percentage of neoplastic cells comprising the bulk of the tumor, as well as host cells, will not survive, while others will attach to the tissue culture treated flask after plating. It is critical that the neurospheres that will form over 1-3 weeks (Figures 1B-E) are transferred to fresh flasks, to separate from differentiated tumor cells and debris.
GBM cells enzymatically dissociated and never cultured (step 1.10) can be cryopreserved as a backup source of cells to culture in alternative media, in case the neurosphere culture fails. We have successfully obtained neurosphere cultures from such frozen stocks, as well as monolayer cells growing in 2% FBS/NMGF.
Conceptually, &#34;cancer stem cell&#34; is a work in progress and this emerging field will benefit from additional clarification, since the clinical implications are considerable, particularly in the generation of tumor heterogeneity, plasticity, and resistance to therapy19,20. In addition to being vital for generating patient-specific GBM animal models, the neurosphere cultures are also valuable for in vitro studies such as alteration in cell signaling and gene expression in response to growth factors, hypoxia, and pharmacological agents11,21. We have opted for using cross-sections of formalin fixed and paraffin embedded neurospheres, preserving the 3D architecture, to study protein expression and post-translational modifications by immunohistochemistry11, due to the superior subcellular localization in relation to the more common method of labeling and imaging the whole sphere.
It has been shown that not all cells within neurospheres derived from adult mammalian brain are stem cells22. Similarly, the neurospheres cultured from GBM tumors are likely not clonal, due to the presence of more differentiated cancer progenitor cells and self-aggregation, known to occur at high cell densities23, which is considered a limitation of this method by some. To favor enrichment for long term self-renewing stem cells, as opposed to just progenitors which can transiently grow as neurospheres22, the primary neurospheres are dissociated for secondary neurosphere formation, and further passaged for a minimum of 10 passages, roughly equivalent to 2 months in continuous culture, which is an indication of a population enriched in stem cells22. In our experience, GBM neurosphere cultures that achieve that mark can continue to be expanded as neurospheres indefinitely. Tumor grade matters, since we have obtained successful cultures from GBMs and anaplastic astrocytomas, WHO grade IV and III, respectively, but not from lower grade gliomas.
The most prevalent method of culturing glioblastoma cells, in traditional growth medium supplemented with 10% FBS, leads to considerable genomic and phenotypic divergence from the original tumors&#160;4. On the other hand, neurosphere cultures are a stable and long term source of cells presenting cancer stem cell phenotype4. The neurosphere method has become increasingly popular for the enrichment of CSC in long term cultures for orthotopic mouse xenograft models, despite not being successful for all high grade astrocytoma samples, which represents the main weakness of this method. Studies to understand how molecular characteristics of the parental tumors can affect neurosphere formation are underway. Exploration of practical alternative methods to culture high grade gliomas, followed by extensive validation are granted, given the momentous advantages of having patient specific GBM models, as we advance into an era of personalized medicine, fuelled by the accessibility of &#34;omics&#34; information and increased numbers of potential targeted therapies.

Glioblastoma (GBM), a WHO grade IV astrocytoma, is the most prevalent and aggressive primary brain tumor. Diverse developmental phenotypes are adopted by GBM tumor cells, including cells exhibiting &#34;cancer stem cell&#34; (CSC) characteristics, such as the expression of neural stem cell (NSC) markers, long term self-renewal, and the potential to give rise to more differentiated cells expressing astrocytic markers and forming the bulk of the tumor1-3. While clarification is still needed regarding CSC molecular identity and clinical implications, the focus of the present work is on the operational definition of CSC: long term self-renewal in vitro&#160;and the ability to differentiate and reproduce the original tumor upon orthotopic implantation in immunocompromised rodents.
Glioblastoma cells have been cultured for decades in traditional medium containing 10% fetal bovine serum (FBS)&#160;and several high passage commercially available serum cultured GBM cell lines are tumorigenic in immunocompromised rodents, but there is considerable genomic and molecular divergence from the original tumor4, limiting their use as clinically relevant models. More recently, cells with stem/progenitor phenotype responsive to EGF and bFGF were identified in GBMs2. Subsequently, dissociated GBM tumor samples were cultured in a serum-free medium3, originally formulated for the selection and expansion of neural stem cells from the adult mammalian brain5. These culture conditions hinder the growth of most nonneoplastic and more differentiated tumor cell populations, while favoring the growth of stem and progenitor cells as floating multicellular spheroids, or neurospheres3, mimicking the behavior of adult mammalian neural stem cells5. Comprehensive side by side comparison of primary GBM cells cultured in either neurosphere medium supplemented with growth factors (NMGF) or in the traditional growth medium supplemented with 10% FBS, revealed that the GBM neurospheres were tumorigenic, presented multilineage differentiation potential, and preserved the genotype of the original tumor, in contrast to the 10% FBS cultures which were not tumorigenic at low passages and considerably diverged from the original tumors at late passages4.
Isolation of CSC from dissociated GBM tumors by cell sorting based on the expression of putative CSC marker CD133 has also been proposed6,7, but further work indicated that the CSC phenotype is not definitively associated with the expression of such markers8-10, decreasing the initial enthusiasm for this strategy, whereas new markers are still being tested10. The unavailability to date of a validated set of markers defining CSC, along with the goal of large scale amplification of these cells for preclinical studies, renders the use of cell sorting impractical for routine CSC-enriched cultures. GBM cells selected by the ability to grow as neurospheres in NMGF invariably express neural stem cell markers. We have observed that Sox2 and nestin are ubiquitously expressed in neurosphere cultures, while CD133 protein is present in a subset of the GBM neurospheres (unpublished data and reference11).
Several laboratories are pursuing neurosphere cultures from glioblastoma tumors using the same general approach of enzymatic dissociation and culturing in serum-free medium supplemented with growth factors3,4,11-14, while other colleagues have reported attempts to grow long term neurosphere cultures from GBM samples without success . The general method for enzymatic dissociation and neurosphere culture of high grade gliomas presented here is similar to what has been outlined in the above publications. We have optimized the protocol based on our experience of dissociating and culturing over 100 GBM samples. The efficiency of obtaining long-term neurosphere cultures from fresh GBM samples applying the protocol presented here is over 40%, similar to the few reports showing efficiency data3,15, leading to the exploration of alternative protocols such as culturing cells continually or intermittently in serum-free medium in the presence of EGF and bFGF as monolayers on surfaces coated with ECM protein16,17. Neurosphere cultures are still the most validated and increasingly popular approach to preserve GBM tumors molecular characteristics and tumorigenic potential3,4,11-14, thus our approach is to attempt neurospheres cultures first, while concomitantly testing alternative methods for culturing GBM cells that fail to form long term self-renewing neurospheres (Figure&#160;1), to increase the representation of GBM tumors that can be used in animal models. Here we present a protocol for culturing neurospheres from GBMs. For cells that fail to form neurospheres, we show a simple modification in the growth medium, as the first attempt to culture tumorigenic cells from nonneurosphere forming GBMs, with promising results and still undergoing extensive validation.

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			<td height="21" style="height:21px;width:216px;">DMEM/F12</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">11330-032</td>
			<td style="width:167px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Trypsin - EDTA 0.05%</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">25300-054</td>
			<td></td>
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		<tr height="60">
			<td height="60" style="height:60px;width:216px;">Hank&#8217;s Balanced Salt Solution, calcium- and magnesium-free</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">14170-120</td>
			<td></td>
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		<tr height="60">
			<td height="60" style="height:60px;width:216px;">Hank&#8217;s Balanced Salt Solution, with calcium and magnesium&#160;</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">24020-117</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Collagenase Type 4</td>
			<td style="width:143px;">Worthington</td>
			<td style="width:119px;">5004188</td>
			<td></td>
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		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Trypsin Inhibitor</td>
			<td style="width:143px;">Sigma</td>
			<td style="width:119px;">T7659</td>
			<td></td>
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		<tr height="21">
			<td height="21" style="height:21px;width:216px;">DNase I</td>
			<td style="width:143px;">Sigma</td>
			<td style="width:119px;">D4527</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">N2 Supplement (100x)</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">17502-048</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;width:216px;">Albumin from Bovine Serum, cell culture grade</td>
			<td style="width:143px;">Sigma</td>
			<td style="width:119px;">A4919</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Gentamicin Reagent Solution</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">15710-064</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Antibiotic/Antimycotic</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">15240-062</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;width:216px;">Recombinant Human FGF-basic</td>
			<td style="width:143px;">PeproTech</td>
			<td style="width:119px;">100-18B</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Recombinant Human EGF</td>
			<td style="width:143px;">PeproTech</td>
			<td style="width:119px;">AF-100-15</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;width:216px;">Lympholyte-Mouse</td>
			<td style="width:143px;">Cedarlane Laboratories Ltd.</td>
			<td style="width:119px;">CL5031</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;width:216px;">Recovery Cell Culture Freezing Medium</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">12648-010</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Sterile Cell Strainer, 40 &#956;m</td>
			<td style="width:143px;">Fisher</td>
			<td style="width:119px;">22363547</td>
			<td></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:216px;">Dulbecco&#39;s Phosphate-Buffered Saline (DPBS), no calcium and no magnesium</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">14190-144</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Fetal bovine serum</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">26140-079</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Trypan Blue Stain, 0.4%</td>
			<td style="width:143px;">Life Technologies</td>
			<td style="width:119px;">15250-061</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Neutral Buffered Formalin</td>
			<td style="width:143px;">Protocol</td>
			<td style="width:119px;">245-684</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Histoplex Tissue Cassettes</td>
			<td style="width:143px;">Thermo Scientific</td>
			<td style="width:119px;">22-146-426</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Rotator</td>
			<td style="width:143px;">Miltenyi BioTec</td>
			<td style="width:119px;">130-090-753</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">GlutaMAX&#160;Supplement</td>
			<td style="width:143px;">Life Technologies</td>
			<td>35050-061</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">KnockOut D-MEM/F12</td>
			<td style="width:143px;">Life Technologies</td>
			<td>12660-012</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Stem Pro Neural Supplement&#160;</td>
			<td style="width:143px;">Life Technologies</td>
			<td>A1058-01</td>
			<td></td>
		</tr>
	</tbody>
</table>

optimization of high grade glioma cell culture from surgical specimens for use in  clinically relevant animal models and 3d immunochemistry

Glioblastomas, the most common and aggressive form of astrocytoma, are refractory to therapy, and molecularly heterogeneous. The ability to establish cell cultures that preserve the genomic profile of the parental tumors, for use in patient specific in vitro and in vivo models, has the potential to revolutionize the preclinical development of new treatments for glioblastoma tailored to the molecular characteristics of each tumor.
Starting with fresh high grade astrocytoma tumors dissociated into single cells, we use the neurosphere assay as an enrichment method for cells presenting cancer stem cell phenotype, including expression of neural stem cell markers, long term self-renewal in vitro, and the ability to form orthotopic xenograft tumors. This method has been previously proposed, and is now in use by several investigators. Based on our experience of dissociating and culturing 125 glioblastoma specimens, we arrived at the detailed protocol we present here, suitable for routine neurosphere culturing of high grade astrocytomas and large scale expansion of tumorigenic cells for preclinical studies. We report on the efficiency of successful long term cultures using this protocol&#160;and suggest affordable alternatives for culturing dissociated glioblastoma cells that fail to grow as neurospheres. We also describe in detail a protocol for preserving the neurospheres 3D architecture for immunohistochemistry. Cell cultures enriched in CSCs, capable of generating orthotopic xenograft models that preserve the molecular signatures and heterogeneity of GBMs, are becoming increasingly popular for the study of the biology of GBMs and for the improved design of preclinical testing of potential therapies.

We have applied the protocol described above to dissociate and culture 125 fresh surgical glioblastoma specimens (Figure 1), 88 newly diagnosed, and 37 recurrent tumors (Table 2), with approved patient consent and under institutional guidelines. The efficiency of the protocol for establishing long term neurosphere cultures was 41.6%, and similar for newly diagnosed tumors and recurrent tumors (Table 2). For some GBM samples, neurospheres form in the first few days (Figures 1B and 1C), while for others longer culturing time is required (Figures 1D and 1E).
Efficiency of neurosphere formation was not exclusively dependent on the level of necrosis in the tissue, as exemplified by the results from a newly diagnosed tumor with high cell density (GBM1) and a recurrent and necrotic tumor (GBM2) processed according to Protocols 1 and 2, both yielding neurosphere cultures (Figure 2).
Testing the tumorigenic potential of each neurosphere culture in immunocompromised mice is the crucial validation of this approach for enrichment of CSCs. Using a protocol similar to previously described18, GBM1 and GBM2 neurospheres were implanted into the brains of immunocompromised mice, under institutional and IACUC animal care guidelines. The xenograft tumors present morphological characteristics of GBMs, such as invasion into the brain parenchyma and necrosis (Figure 2).
GBM3 was dissociated (Figure 1A) and cultured in neurosphere medium (Figures 1D and 1E), and in 2% FBS/NMGF (Figures 1D, 1G, and 1H). Monolayer cells cultured in 2% FBS/NMGF and neurosphere cells cultured in NMGF were dissociated and the same number of cells were implanted in nude mouse, using the same procedure as in Figure 2. No differences in survival, tumor growth dynamics, or morphology were observed between the two preimplant culture methods (Figures 3A-C). Tumor growth characteristics do not change up to the latest passage tested, P20 for neurospheres, and P10 for 2% FBS/NMGF. While neural stem cell markers, including Sox2, are downregulated in most primary GBM cells cultured in 10% FBS 3,4,11, NMGF supplemented with 2% FBS allows for the retention of Sox2 expression (Figure 3D).
Neurospheres were processed according to Protocol 4, and labeled with H&#38;E (Figure 4A), anti-Sox2 antibody, showing nuclear localization (Figure 4B), and EGFR antibody, cell membrane localization (Figure 4C). This protocol has been applied to access stimuli-dependent alterations in the expression of nestin, GFAP, and the proliferation marker Ki6711.
Table 2. Efficiency of deriving long term self-renewing neurosphere cultures from GBMs.
<table border="1">
	<tbody>
		<tr>
			<td>Pathology</td>
			<td>n</td>
			<td>Percentage of samples yielding long term self-renewing neurospheres (n)</td>
		</tr>
		<tr>
			<td>Glioblastoma - untreated, first surgery</td>
			<td>88</td>
			<td>42.0% (37)</td>
		</tr>
		<tr>
			<td>Glioblastoma - recurrent</td>
			<td>37</td>
			<td>40.5% (15)</td>
		</tr>
		<tr>
			<td>TOTAL</td>
			<td>125</td>
			<td>41.6% (52)</td>
		</tr>
	</tbody>
</table>
<img alt="Figure 1" fo:content-width="5in" fo:src="/files/ftp_upload/51088/51088fig1highres.jpg" src="/files/ftp_upload/51088/51088fig1.jpg" /> 
	Figure 1. Cell culture from fresh glioblastoma surgical specimens. Fresh tumors are enzymatically dissociated into single cells. Nucleated cell interface from density separation medium is then plated in NMGF. Dissociated neurospheres are plated in NMGF, and typically 1 day after plating there are dead cells, debris, attached single cells, and occasional dividing cells in suspension (A). Neurosphere formation is faster for some cases (B,C), and slower for others (D,E). All neurospheres are dissociated and replated for at least 10 passages, 41.6% GBMs yield long term self-renewing neurospheres. Viable GBM dissociated cells that fail to grow as neurospheres (F) can be transferred to alternative culture conditions, for example 2% FBS/NMGF (G,H). Bar (A), 100 &#956;m, applies to all images. <a href="https://www.jove.com/files/ftp_upload/51088/51088fig1highres.jpg" target="_blank"> Click here to view larger image.</a>
<img alt="Figure 2" fo:content-width="5in" fo:src="/files/ftp_upload/51088/51088fig2highres.jpg" src="/files/ftp_upload/51088/51088fig2.jpg" /> 
	Figure 2. Neurosphere generation and orthotopic mouse xenografts from GBM tumors. A tumor sample presenting high cell density (GBM1) and a tumor with high necrotic content (GBM2) were dissociated and neurospheres cultured for 10 passages according to Protocols 1 and 2. Immunocompromised mice were implanted with 3 x 105 dissociated neurosphere cells and sacrificed when moribund. Mouse brains were formalin fixed and paraffin embedded for H&#38;E staining and immunohistochemistry detection of human markers, human mitochondria (hMit) or major histocompatibility class I subunit HLA-A (MHC-I). <a href="https://www.jove.com/files/ftp_upload/51088/51088fig2highres.jpg" target="_blank"> Click here to view larger image.</a>
<img alt="Figure 3" fo:content-width="5in" fo:src="/files/ftp_upload/51088/51088fig3highres.jpg" src="/files/ftp_upload/51088/51088fig3.jpg" /> 
	Figure 3. Similar tumor growth in mice implanted intracranially with GBM3 cells cultured as neurospheres in NMGF or as monolayers in 2% FBS/NMGF. (A) Kaplan-Meier survival curves for GBM3 cultured as either neurospheres in NMGF or monolayers in 2%FBS/NMGF (both passage &#60;10) show no difference in survival (n=10, p=0.7174, log-rank test). (B) Tumor growth monitored by live bioluminescence imaging (BLI) show no significant difference in tumor growth dynamics between the two groups. (C) Tumor morphology is indistinguishable for 4 GBM3 xenografts, 2 cultured in NMGF and 2 cultured in 2% FBS/NMGF. MHC-I stain as described for Figure 2. Scale, 600 &#956;m. (D) Western blot showing the stem cell maker Sox2 expression retained in 2% FBS/NMGF cultures used to initiate the xenograft tumors (A-C). <a href="https://www.jove.com/files/ftp_upload/51088/51088fig3highres.jpg" target="_blank"> Click here to view larger image.</a>
<img alt="Figure 4" fo:content-width="5in" fo:src="/files/ftp_upload/51088/51088fig4highres.jpg" src="/files/ftp_upload/51088/51088fig4.jpg" /> 
	Figure 4. Analysis of protein expression in neurosphere sections by immunohistochemistry. Neurosphere cultures were formalin-fixed and paraffin embedded as described in Procedure 4, and stained with H&#38;E (A), anti-Sox2 antibody (B), and anti-EGFR antibody (C). DAB substrate was used to visualize (B,C). Bar, 20 &#956;m. <a href="https://www.jove.com/files/ftp_upload/51088/51088fig4highres.jpg" target="_blank">Click here to view larger image.</a>

Watch this Scientific Journal Video about Optimization of High Grade Glioma Cell Culture from Surgical Specimens for Use in  Clinically Relevant Animal Models and 3D Immunochemistry at JoVE.com

Optimization of High Grade Glioma Cell Culture from Surgical Specimens for Use in  Clinically Relevant Animal Models and 3D Immunochemistry

Protocol for propagation of dissociated high grade glioma surgical specimens in serum-free neurosphere medium to select for cells with cancer stem cell phenotype. For specimens that fail to grow as neurospheres, an alternative protocol is suggested. A paraffin embedding technique for maintaining the 3D neurosphere architecture for immunocytochemistry is described.

Glioblastomas, the most common and aggressive form of astrocytoma, are refractory to therapy, and molecularly heterogeneous. The ability to establish cell ...

optimization-high-grade-glioma-cell-culture-from-surgical-specimens

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14.9K vues.  Henry Ford Hospital. Protocole pour la propagation des spécimens chirurgicaux à haute teneur dissociés de gliome dans le milieu sans sérum de neurosphère pour sélectionner pour des cellules avec le phénotype de cellules souches cancéreuses. Pour les spécimens qui ne se développent pas en tant que neurosphères, un protocole alternatif est suggéré. Une technique de incorporation de paraffine pour maintenir l’architecture 3D de neurosphère pour immunocytochemistry est décrite.

Vidéo: Optimization of High Grade Glioma Cell Culture from Surgical Specimens for Use in  Clinically Relevant Animal Models and 3D Immunochemistry

Implantation of Radiotelemetry Transmitters Yielding Data on ECG, Heart Rate, Core Body Temperature and Activity in Free-moving Laboratory Mice

The laboratory mouse is the animal species of choice for most biomedical research, in both the academic sphere and the pharmaceutical industry. Mice are a manageable size and relatively easy to house. These factors, together with the availability of a wealth of spontaneous and experimentally induced mutants, make laboratory mice ideally suited to a wide variety of research areas.
In cardiovascular, pharmacological and toxicological research, accurate measurement of parameters relating to the circulatory system of laboratory animals is often required. Determination of heart rate, heart rate variability, and duration of PQ and QT intervals are based on electrocardiogram (ECG) recordings. However, obtaining reliable ECG curves as well as physiological data such as core body temperature in mice can be difficult using conventional measurement techniques, which require connecting sensors and lead wires to a restrained, tethered, or even anaesthetized animal. Data obtained in this fashion must be interpreted with caution, as it is well known that restraining and anesthesia can have a major artifactual influence on physiological parameters1, 2.
Radiotelemetry enables data to be collected from conscious and untethered animals. Measurements can be conducted even in freely moving animals, and without requiring the investigator to be in the proximity of the animal. Thus, known sources of artifacts are avoided, and accurate and reliable measurements are assured. This methodology also reduces interanimal variability, thus reducing the number of animals used, rendering this technology the most humane method of monitoring physiological parameters in laboratory animals3, 4. Constant advancements in data acquisition technology and implant miniaturization mean that it is now possible to record physiological parameters and locomotor activity continuously and in realtime over longer periods such as hours, days or even weeks3, 5.
Here, we describe a surgical technique for implantation of a commercially available telemetry transmitter used for continuous measurements of core body temperature, locomotor activity and biopotential (i.e. onelead ECG), from which heart rate, heart rate variability, and PQ and QT intervals can be established in freeroaming, untethered mice. We also present pre-operative procedures and protocols for post-operative intensive care and pain treatment that improve recovery, well-being and survival rates in implanted mice5, 6.

A surgical technique for implantation of commercially available telemetry transmitters used for continuous measurement of biopotential (one-lead ECG), heart rate, core body temperature and locomotor activity in freely moving mice is shown. Recommendations and protocols for post-operative care and pain relief, improving recovery, well being and survival rate are also presented.

The laboratory mouse is the animal species of choice for most biomedical research, in both the academic sphere and the pharmaceutical industry. Mice are a ...

Improved Protocol For Laser Microdissection Of Human Pancreatic Islets From Surgical Specimens

Laser microdissection (LMD) is a technique that allows the recovery of selected cells and tissues from minute amounts of parenchyma 1,2. The dissected cells can be used for a variety of investigations, such as transcriptomic or proteomic studies, DNA assessment or chromosomal analysis 2,3. An especially challenging application of LMD is transcriptome analysis, which, due to the lability of RNA 4, can be particularly prominent when cells are dissected from tissues that are rich of RNases, such as the pancreas. A microdissection protocol that enables fast identification and collection of target cells is essential in this setting in order to shorten the tissue handling time and, consequently, to ensure RNA preservation. 
Here we describe a protocol for acquiring human pancreatic beta cells from surgical specimens to be used for transcriptomic studies 5. Small pieces of pancreas of about 0.5-1 cm3 were cut from the healthy appearing margins of resected pancreas specimens, embedded in Tissue-Tek O.C.T. Compound, immediately frozen in chilled 2-Methylbutane, and stored at -80 &deg;C until sectioning. Forty serial sections of 10 &mu;m thickness were cut on a cryostat under a -20 &deg;C setting, transferred individually to glass slides, dried inside the cryostat for 1-2 min, and stored at -80 &deg;C. 
Immediately before the laser microdissection procedure, sections were fixed in ice cold, freshly prepared 70% ethanol for 30 sec, washed by 5-6 dips in ice cold DEPC-treated water, and dehydrated by two one-minute incubations in ice cold 100% ethanol followed by xylene (which is used for tissue dehydration) for 4 min; tissue sections were then air-dried afterwards for 3-5 min. Importantly, all steps, except the incubation in xylene, were performed using ice-cold reagents - a modification over a previously described protocol 6. utilization of ice cold reagents resulted in a pronounced increase of the intrinsic autofluorescence of beta cells, and facilitated their recognition. For microdissection, four sections were dehydrated each time: two were placed into a foil-wrapped 50 ml tube, to protect the tissue from moisture and bleaching; the remaining two were immediately microdissected. This procedure was performed using a PALM MicroBeam instrument (Zeiss) employing the Auto Laser Pressure Catapulting (AutoLPC) mode. The completion of beta cell/islet dissection from four cryosections required no longer than 40-60 min. Cells were collected into one AdhesiveCap and lysed with 10 &mu;l lysis buffer. Each single RNA specimen for transcriptomic analysis was obtained by combining 10 cell microdissected samples, followed by RNA extraction using the Pico Pure RNA Isolation Kit (Arcturus). This protocol improves the intrinsic autofluorescence of human beta cells, thus facilitating their rapid and accurate recognition and collection. Further improvement of this procedure could enable the dissection of phenotypically different beta cells, with possible implications for better understanding the changes associated with type 2 diabetes.

Laser microdissection is a technique that allows the recovery of selected cells from minute amounts of parenchyma. Here we describe a protocol for acquiring human pancreatic islets from surgical specimens to be used for transcriptomic studies. Our protocol improves the intrinsic autofluorescence of human beta cells, thus facilitating their collection.

Laser microdissection (LMD) is a technique that allows the recovery of selected cells and tissues from minute amounts of parenchyma 1,2. The dissected ...

High-frequency Ultrasound Imaging of Mouse Cervical Lymph Nodes

High-frequency ultrasound (HFUS) is widely employed as a non-invasive method for imaging internal anatomic structures in experimental small animal systems. HFUS has the ability to detect structures as small as 30 &#181;m, a property that has been utilized for visualizing superficial lymph nodes in rodents in brightness (B)-mode. Combining power Doppler with B-mode imaging allows for measuring circulatory blood flow within lymph nodes and other organs. While HFUS has been utilized for lymph node imaging in a number of mouse&#160; model systems, a detailed protocol describing HFUS imaging and characterization of the cervical lymph nodes in mice has not been reported. Here, we show that HFUS can be adapted to detect and characterize cervical lymph nodes in mice. Combined B-mode and power Doppler imaging can be used to detect increases in blood flow in immunologically-enlarged cervical nodes. We also describe the use of B-mode imaging to conduct fine needle biopsies of cervical lymph nodes to retrieve lymph tissue for histological&#160; analysis. Finally, software-aided steps are described to calculate changes in lymph node volume and to visualize changes in lymph node morphology following image reconstruction. The ability to visually monitor changes in cervical lymph node biology over time provides a simple and powerful technique for the non-invasive monitoring of cervical lymph node alterations in preclinical mouse models of oral cavity disease.

This protocol describes the application of high-frequency ultrasound (HFUS) for imaging mouse cervical lymph nodes. This technique optimizes visualization and quantification of cervical lymph node morphology, volume and blood flow. Image-guided biopsy of cervical lymph nodes and processing of lymph tissue for histological evaluation is also demonstrated.

High-frequency ultrasound (HFUS) is widely employed as a non-invasive method for imaging internal anatomic structures in experimental small animal ...

Use of Ultra-high Field MRI in Small Rodent Models of Polycystic Kidney Disease for In Vivo Phenotyping and Drug Monitoring

Several in vivo pre-clinical studies in Polycystic Kidney Disease (PKD) utilize orthologous rodent models to identify and study the genetic and molecular mechanisms responsible for the disease, and are very convenient for rapid drug screening and testing of promising therapies. A limiting factor in these studies is often the lack of efficient non-invasive methods for sequentially analyzing the anatomical and functional changes in the kidney. Magnetic resonance imaging (MRI) is the current gold standard imaging technique to follow autosomal dominant polycystic kidney disease (ADPKD) patients, providing excellent soft tissue contrast and anatomic detail and allowing Total Kidney Volume (TKV) measurements.A major advantage of MRI in rodent models of PKD is the possibility for in vivo imaging allowing for longitudinal studies that use the same animal and therefore reducing the total number of animals required. In this manuscript, we will focus on using Ultra-high field (UHF) MRI to non-invasively acquire in vivo images of rodent models for PKD. The main goal of this work is to introduce the use of MRI as a tool for in vivo phenotypical characterization and drug monitoring in rodent models for PKD.

Use of Ultra-high Field MRI in Small Rodent Models of Polycystic Kidney Disease for In Vivo Phenotyping and Drug Monitoring

The use of ultra-high field MRI as a non-invasive way to obtain phenotypic information of rodent models for polycystic kidney disease and to monitor interventions is described. Compared with the traditional histological approach, MRI images can be acquired in vivo, allowing for longitudinal follow-up.

Several in vivo pre-clinical studies in Polycystic Kidney Disease (PKD) utilize orthologous rodent models to identify and study the genetic and molecular ...

Implementation of In Vitro Drug Resistance Assays: Maximizing the Potential for Uncovering Clinically Relevant Resistance Mechanisms

Although targeted therapies are initially effective, resistance inevitably emerges. Several methods, such as genetic analysis of resistant clinical specimens, have been applied to uncover these resistance mechanisms to facilitate follow-up care. Although these approaches have led to clinically relevant discoveries, difficulties in attaining the relevant patient material or in deconvoluting the genomic data collected from these specimens have severely hampered the path towards a cure. To this end, we here describe a tool for expeditious discovery that may guide improvement in first-line therapies and alternative clinical management strategies. By coupling preclinical in vitro or in vivo drug selection with next-generation sequencing, it is possible to identify genomic structural variations and/or gene expression alterations that may serve as functional drivers of resistance. This approach facilitates the spontaneous emergence of alterations, enhancing the probability that these mechanisms may be observed in the patients. In this protocol we provide guidelines to maximize the potential for uncovering single nucleotide variants that drive resistance using adherent lines.

Implementation of In Vitro Drug Resistance Assays: Maximizing the Potential for Uncovering Clinically Relevant Resistance Mechanisms

Drug resistance to targeted therapeutics is widespread and the need to identify mechanisms of resistance--prior to or following clinical onset--is critical for guiding alternative clinical management strategies. Here, we present a protocol to couple derivation of drug-resistant lines in vitro with sequencing to expedite discovery of these mechanisms.

Although targeted therapies are initially effective, resistance inevitably emerges. Several methods, such as genetic analysis of resistant clinical ...

Surgical Models of Gastroesophageal Reflux with Mice

Multiple surgical procedures have been reported to induce gastroesophageal reflux in animals. Herein, we report three surgical models with mice aiming to induce reflux of gastric contents, duodenal contents or mixed contents. Surgical procedures and general principles have been described in detail. A researcher with surgical experience should be able to grasp the technique after a short period of practice. After surgery, most mice can survive and develop reflux esophagitis similar to that in humans. However, it should be noted that histological differences between mouse and human esophagus are the inherent limitations of these surgical models. If used for research on Barrett&#8217;s esophagus and adenocarcinoma, these procedures may need to be combined with genetic modifications.

This article demonstrates surgical procedures of gastroesophageal reflux with mice. These models are useful tools for research on mechanisms and treatment of gastroesophageal reflux disease and potentially Barrett&#8217;s esophagus and esophageal adenocarcinoma.

Multiple surgical procedures have been reported to induce gastroesophageal reflux in animals. Herein, we report three surgical models with mice aiming to ...

Cutaneous Surgical Denervation:  A Method for Testing the Requirement for Nerves in Mouse Models of Skin Disease

Cutaneous somatosensory nerves function to detect diverse stimuli that act upon the skin. In addition to their established sensory roles, recent studies have suggested that nerves may also modulate skin disorders including atopic dermatitis, psoriasis and cancer. Here, we describe protocols for testing the requirement for nerves in maintaining a cutaneous mechanosensory organ, the touch dome (TD). Specifically, we discuss methods for genetically labeling, harvesting and visualizing TDs by whole-mount staining, and for performing unilateral surgical denervation on mouse dorsal back skin. Together, these approaches can be used to directly compare TD morphology and gene expression in denervated as well as sham-operated skin from the same animal. These methods can also be readily adapted to examine the requirement for nerves in mouse models of skin pathology. Finally, the ability to repeatedly sample the skin provides an opportunity to monitor disease progression at different stages and times after initiation.

This article includes detailed protocols for genetic labeling of mouse skin, surgical denervation, skin biopsy and visualizing labeled epithelia by whole-mount &#946;-galactosidase staining. These methods can be used to test the requirement for nerves in mouse models of normal and pathological skin.

Cutaneous somatosensory nerves function to detect diverse stimuli that act upon the skin. In addition to their established sensory roles, recent studies ...

A Model to Simulate Clinically Relevant Hypoxia in Humans

In case of apnea, arterial partial pressure of oxygen (pO2) decreases, while partial pressure of carbon dioxide (pCO2) increases. To avoid damage to hypoxia sensitive organs such as the brain, compensatory circulatory mechanisms help to maintain an adequate oxygen supply. This is mainly achieved by increased cerebral blood flow. Intermittent hypoxia is a commonly seen phenomenon in patients with obstructive sleep apnea. Acute airway obstruction can also result in hypoxia and hypercapnia. Until now, no adequate model has been established to simulate these dynamics in humans. Previous investigations focusing on human hypoxia used inhaled hypoxic gas mixtures. However, the resulting hypoxia was combined with hyperventilation and is therefore more representative of high altitude environments than of apnea. Furthermore, the transferability of previously performed animal experiments to humans is limited and the pathophysiological background of apnea induced physiological changes is poorly understood. In this study, healthy human apneic divers were utilized to mimic clinically relevant hypoxia and hypercapnia during apnea. Additionally, pulse-oximetry and Near Infrared Spectroscopy (NIRS) were used to evaluate changes in cerebral and peripheral oxygen saturation before, during, and after apnea.

Hypoxia simulation in humans has usually been performed by inhaling hypoxic gas mixtures. For this study, apneic divers were used to simulate dynamic hypoxia in humans. Additionally, physiological changes in desaturation and re-saturation kinetics were evaluated with non-invasive tools such as Near-Infrared-Spectroscopy (NIRS) and peripheral oxygenation saturation (SpO2).

In case of apnea, arterial partial pressure of oxygen (pO2) decreases, while partial pressure of carbon dioxide (pCO2) increases. To avoid damage to ...

Assessment of the Anticoagulant and Anti-inflammatory Properties of Endothelial Cells Using 3D Cell Culture and Non-anticoagulated Whole Blood

In vivo, endothelial cells are crucial for the natural anticoagulation of circulating blood. Consequently, endothelial cell activation leads to blood coagulation. This phenomenon is observed in many clinical situations, like organ transplantation in the presence of pre-formed anti-donor antibodies, including xenotransplantation, as well as in ischemia/reperfusion injury. In order to reduce animal experimentation according to the 3R standards (reduction, replacement and refinement), in vitro models to study the effect of endothelial cell activation on blood coagulation would be highly desirable. However, common flatbed systems of endothelial cell culture provide a surface-to-volume ratio of 1 - 5 cm2 of endothelium per mL of blood, which is not sufficient for natural, endothelial-mediated anticoagulation. Culturing endothelial cells on microcarrier beads may increase the surface-to-volume ratio to 40 - 160 cm2/mL. This increased ratio is sufficient to ensure the &#34;natural&#34; anticoagulation of whole blood, so that the use of anticoagulants can be avoided. Here an in vitro microcarrier-based system is described to study the effects of genetic modification of porcine endothelial cells on coagulation of whole, non-anticoagulated human blood. In the described assay, primary porcine aortic endothelial cells, either wild type (WT) or transgenic for human CD46 and thrombomodulin, were grown on microcarrier beads and then exposed to freshly drawn non-anticoagulated human blood. This model allows for the measurement and quantification of cytokine release as well as activation markers of complement and coagulation in the blood plasma. In addition, imaging of activated endothelial cell and deposition of immunoglobulins, complement- and coagulation proteins on the endothelialized beads were performed by confocal microscopy. This assay can also be used to test drugs which are supposed to prevent endothelial cell activation and, thus, coagulation. On top of its potential to reduce the number of animals used for such investigations, the described assay is easy to perform and consistently reproducible.

We present an in vitro model which allows the study and analysis of coagulation in whole, non-anticoagulated blood. Anticoagulation in the system depends on the natural anticoagulation effect of healthy endothelial cells and endothelial cell activation will result in clotting.

In vivo, endothelial cells are crucial for the natural anticoagulation of circulating blood. Consequently, endothelial cell activation leads to blood ...

Isolation and Culture of Resident Cardiac Macrophages from the Murine Sinoatrial and Atrioventricular Node

Resident cardiac macrophages have been demonstrated to facilitate the electrical conduction in the heart. The physiologic heart rhythm is initiated by electrical impulses generated in sinoatrial node (SAN) and then conducted to ventricles via atrioventricular node (AVN). To further study the role of resident macrophages in cardiac conduction system, a proper isolation of resident macrophages from SAN and AVN is necessary, but it remains challenging. Here, we provide a protocol for the reliable microdissection of the SAN and AVN in murine hearts followed by the isolation and culture of resident macrophages.
Both, SAN which is located at the junction of the crista terminalis with the superior vena cava, and AVN which is located at the apex of the triangle of Koch, are identified and microdissected. Correct location is confirmed by histologic analysis of the tissue performed with Masson's trichrome stain and by anti-HCN4.
Microdissected tissues are then enzymatically digested to obtain single cell suspensions followed by the incubation with a specific panel of antibodies directed against cell-type specific surface markers. This allows to identify, count, or isolate different cell populations by fluorescent activated cell sorting. To differentiate cardiac resident macrophages from other immune cells in the myocardium, especially recruited monocyte-derived macrophages, a delicate devised gating strategy is needed. First, lymphoid lineage cells are detected and excluded from further analysis. Then, myeloid cells are identified with resident macrophages being determined by high expression of both CD45 and CD11b, and low expression of Ly6C. With cell sorting, isolated cardiac macrophages can then be cultivated in vitro over several days for further investigation. We, therefore, describe a protocol to isolate cardiac resident macrophages located within the cardiac conduction system. We discuss pitfalls in microdissecting and digesting SAN and AVN, and provide a gating strategy to reliably identify, count and sort cardiac macrophages by fluorescence-activated cell sorting.

The protocol presented here provides a step-by-step approach for the isolation of cardiac resident macrophages from the sinoatrial node (SAN) and atrioventricular node (AVN) region of mouse hearts.

Resident cardiac macrophages have been demonstrated to facilitate the electrical conduction in the heart. The physiologic heart rhythm is initiated by ...