We are grateful to Gabriele Allies for excellent technical assistance. We thank the University Ulm Medical Faculty for the use of the FACS Core Facility and the Institut f&#252;r Molekulare und Zellul&#228;re Anatomie for using the confocal microscope. We thank S. Hayashi for the esg-Gal4, UAS-GFP fly line. This project is funded by the Federal Ministry of Education and Research (BMBF, Forschungskern SyStaR). A.T. is supported by SFB 1074 (Project A2). A.T. and G.A. are supported by the Deutsche Forschungsgemeinschaft (DFG, FE578/3-1). H.M.T. is a member of the International Graduate School in Molecular Medicine Ulm (GSC 270).

NOTE: If this protocol is used for the first time to isolate ISCs by FAC sorting, the following controls are mandatory in order to initially set the FACS parameters properly: Dissociated cells from wild type (e.g. w1118) Drosophila midguts without Sytox. Dissociated cells from wild type (e.g. w1118) Drosophila midguts with Sytox (see Step 3.6). Dissociated cells from midguts of the esg-Gal4, UAS-GFP fly line without Sytox.
1. Preparation of Solutions and Dishes for Gut Dissection
<ol>
	<li>Prepare 4-6 vials each containing 40 female flies from the esg-Gal4, UAS-GFP fly line.</li>
	<li>From a 10x PBS stock solution prepare 500 ml 1x PBS (1.8 mM NaH2PO4&#183;H2O, 8.4 mM Na2HPO4&#183;2H2O, 175 mM NaCl, adjust pH to 7.4).</li>
	<li>Prepare a 3.5% agarose solution in 1x PBS (3.5 g electrophoresis grade agarose in 100 ml 1x PBS). Prepare dissection plates by pouring this solution into petri dishes (diameter 8.5 cm) to cover the bottom. The agarose layer prevents damaging the tips of the forceps during the dissection procedure. After the gel has solidified store the dissection plates at 4 &#176;C.</li>
	<li>Prepare 300 ml of 1x PBS + 1% BSA fresh before dissecting and place the bottle on ice or at 4 &#176;C.</li>
	<li>Turn on centrifuge and let it cool to 4 &#176;C.</li>
	<li>Flame the tips of 2 glass Pasteur pipettes to smoothen the edges.</li>
	<li>Clean two pairs of forceps and one razor blade with 70% ethanol.</li>
	<li>Place four to six 1.5 ml microcentrifuge tubes for collecting dissected midguts on ice.</li>
</ol>
2. Preparation of the Gastrointestinal Tract and Dissection of the Midgut
<ol>
	<li>Anesthetize flies from one vial (40 flies) with CO2 on a standard fly bed, decapitate all flies using a razor blade and transfer them to the dissection dish. Pour cold 1x PBS/1% BSA solution into the dissection dish to cover the agarose gel. The flies will float.</li>
	<li>Grab the fly abdomen with one pair of forceps, while holding the thorax with the other pair of forceps. Separate the thorax from the abdomen. The gut will be visible and the foregut/crop will most likely still be connected to the thorax.</li>
	<li>Grab the gut and pull it out of the thorax. To unfold the gut, grab the crop and pull the gut slightly anteriorly away from the abdomen.</li>
	<li>Grab the posterior end of the abdomen with one pair of forceps and the edge of the anteriorly open cuticle with the other pair of forceps. Be careful not to destroy the protruding gut tissue. Pull the posterior end away to break the cuticle and continue pulling posteriorly very gently until the entire gut has been pulled out of the abdominal cavity. The crop may have to be removed beforehand if it is too large to fit through the body cavity.</li>
	<li>Remove the foregut, Malpighian tubules, hindgut and ovaries leaving the bare midgut.</li>
	<li>Using a glass Pasteur pipette, transfer the batch of dissected midguts to a 1.5 ml microcentrifuge tube containing cold 1x PBS/1% BSA solution and keep the tube on ice. The samples must be processed within 2 hr.</li>
	<li>After the dissection of an entire batch is complete, rinse the dissection dish with double distilled water to wash off left over debris. Start dissecting the next batch of midguts (repeat Steps 2.1&#8211;2.7). Dissect as many batches as possible within 2 hr, then proceed to Step 3.1.</li>
</ol>
3. Digestion of the Gut Tissue to Harvest Cells for FAC Sorting
<ol>
	<li>Remove the 1x PBS/1% BSA solution from the midguts and add 500 &#181;l of 0.5% Trypsin-EDTA solution to each sample.</li>
	<li>Vortex well for 20 sec and incubate the samples by gentle rocking/rotating at 20 rpm at room temperature for 25-30 min.</li>
	<li>Vortex again after about 30 min and let the intact midgut tissue sink to the bottom of the tube. Carefully remove the cells that are in suspension with a flamed glass Pasteur pipette and filter them through a 35 &#181;m nylon mesh into a fresh 1.5 ml microcentrifuge tube.</li>
	<li>Spin the cells down at 100 x g for 5 min at 4 &#176;C. Of note, when starting the digest, a cell pellet might not be visible at first but will become visible as the tissue digest progresses.
	<ol>
		<li>Carefully transfer the Trypsin solution back to the original sample tube containing the remaining intact midgut tissue. Avoid transferring too many cells from the pellet.</li>
		<li>Gently re-suspend the cell pellet in 400 &#181;l of cold 1x PBS/1% BSA. Keep the microcentrifuge tubes containing the dissociated cells on ice and cover the tubes with aluminum foil to protect the cells from light.</li>
		<li>Vortex the Trypsin solution containing the remaining intact midgut tissue again and place the samples onto the rocker for another 30 min at room temperature.</li>
	</ol>
	</li>
	<li>Repeat steps 3.3 to 3.4.3 until all of the midgut tissue has been digested. Combine the dissociated cells from all microcentrifuge tubes into one microcentrifuge tube. This may require a centrifugation step as in 3.4, since the volume of all cell suspensions combined may exceed 1.5 ml. Keep the cell suspension on ice and protect the cells from light.</li>
	<li>Spin the dissociated cells down at 100 x g for 5 min at 4 &#176;C. Carefully remove as much of the supernatant as possible leaving approximately 50-100 &#181;l of the 1x PBS/1% BSA solution in the microcentrifuge tube. Gently resuspend the dissociated cells in 800 &#181;l 1x PBS/1% BSA containing Sytox (1:20,000).</li>
	<li>Transfer the cell suspension to a 5 ml round bottom Falcon tube by filtering the cells through a cell strainer snap cap (35 &#181;m nylon mesh). Always keep cell samples on ice and protected from light. The cells are now ready to be sorted.</li>
	<li>Pipette 600 &#181;l of RNAlater solution into each microcentrifuge tube into which the cells will be sorted for subsequent RNA isolation. For other downstream applications the cells can be collected in a different solution, e.g. in sterile PBS.</li>
</ol>
4. FAC Sorting to Isolate Intestinal Stem Cells
<ol>
	<li>Switch on the flow cytometry instrument at least one hour prior to sorting. Make sure that the fluidic system is free of air bubbles.</li>
	<li>Choose the 70 &#181;m nozzle size to inject the cells into the sheath fluid stream.</li>
	<li>Adjust the amplitude of the core fluid stream so that the gap value corresponds to the reference value (6-7, when using the 70 &#181;m nozzle). Let the core fluid stream stabilize before starting to sort.</li>
	<li>Follow this order when initially setting the parameters for sorting:
	<ol>
		<li>Load the dissociated cells obtained from wild type guts. First, adjust the FSC and SSC voltages to plot the cells in the center of the scatter plot. Second, adjust the FITC (GFP) voltage so that all cells are plotted below 102 on the logarithmic x-axis. Setting the FITC parameter sets the limit for autofluorescence.</li>
		<li>Load the dissociated cells obtained from wild type guts with Sytox added. Adjust the Pacific Blue voltage value and gate to identify and separate living cells from dead, Sytox-positive cells in the Pacific Blue vs. FSC-A scatter plot.</li>
		<li>Load the dissociated cells obtained from the esg-Gal4, UAS-GFP fly line without Sytox and adjust the FITC voltage to ensure that all GFP-positive cells are plotted within the scatter plot.</li>
	</ol>
	</li>
	<li>Load the dissociated cells obtained from the esg-Gal4, UAS-GFP fly line with Sytox added. Adjust the Pacific Blue voltage value and gate to identify and separate living cells from dead, Sytox-positive cells (gate P1).
	<ol>
		<li>Set the SSC-A and FSC-A gate to identify the GFP-positive cells (based on the histogram plot) as determined by size and granularity (gate P2).</li>
		<li>Set the FSC-H and FSC-W gate to identify and exclude GFP-positive cell doublets based on their size (gate P3).</li>
		<li>Set the SSC-H and the SSC-W gate to identify and exclude GFP-positive cell doublets based on their granularity (gate P4).</li>
		<li>Use gate P4 to depict the GFP-positive cells in a histogram plot that shows the number of cells (count) vs. GFP intensity. Two distinct peaks of GFP-positive cells will be visible. Create a gate for each peak (gates P5 and P6). Gate P5 contains the cell population that is enriched for ISCs and can be sorted separately from the cells in gate P6.</li>
		<li>Back-gate in a contour plot to verify that the two distinct GFP-positive cell populations contain living cells (compare with gate P1) and cells of the correct size (compare with gate P2).</li>
	</ol>
	</li>
	<li>Sort the cells into a 1.5 ml microcentrifuge tube that contains 600 &#181;l of RNAlater solution. The sorting is done at a low flow rate (max. 2.0, 70 &#181;m nozzle, 1,000 events/sec, 70 psi) and employing a two-way purity sort.</li>
	<li>After sorting is complete, immediately vortex the sorted cells briefly and keep the microcentrifuge tubes on ice until proceeding with RNA isolation or other downstream applications.</li>
</ol>

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The authors declare that they have no competing financial interests.

The presented protocol describes a method to isolate ISCs from young and old adult Drosophila midguts, which can subsequently be used for further molecular analyses such as next generation sequencing. FAC sorting of the GFP-positive cell population from the esg-Gal4, UAS-GFP fly line has already been achieved by several groups21,22. However, until now the presence of the two distinct peaks of GFP-positive cells has been either overlooked or undervalued. We show that this separation not only represents two different populations of cell types (ISCs and EBs), but also that the two peaks of GFP-positive cells stay distinctly separate during aging. This observation is highly relevant and valuable to researchers interested in studying stem or progenitor cells during aging. Isolation of ISCs from old midguts has been hampered by the fact that there is no molecular marker combination to identify ISCs in an aged midgut. The only marker that unambiguously identifies ISCs in an old midgut is phospho-histone3 (PH3), since ISCs are the only dividing cells in the midgut12,13. However, PH3 is an unsuitable marker to isolate ISCs since the number of dividing stem cells at any given time point is too low in order to obtain a decent amount of ISCs for subsequent analyses. The fly line esg-Gal4, UAS-GFP is the most common fly line used by researchers who study ISC function, maintenance and differentiation. Our current knowledge on the molecular regulation of ISCs homeostasis is based on studies in which specific molecules and signaling pathways have been manipulated (reviewed in 7). Hence, we still lack knowledge about the endogenous molecular changes that occur during aging. The herein described method closes this gap and is based on the fact that ISCs can be isolated based on their size, granularity and GFP intensity from adult midguts at any time point during aging.
While establishing and optimizing this method we have found the following steps to be critical for a reliable outcome. Approximately 200 guts need to be dissected in order to obtain a good amount of ISCs for FAC sorting. The speed of dissection is crucial and depends on the individual&#8217;s practice. A trained individual can dissect 40 guts within 20&#8211;30 min. Since GFP is also expressed in the Malpighian tubules in the esg-Gal4, UAS-GFP fly line, it is essential to completely remove the Malpighian tubules from the midgut. The dissected midguts must be kept in a cool environment to avoid tissue degradation and reduce RNAse activity in the tissue. Therefore, the dissected midguts must be transferred from the dissecting dish into microcentrifuge tubes containing cold 1x PBS/1% BSA solution after a maximum of 20-30 min and kept on ice. However, the dissected midguts should not be left on ice for more than 2 hr before starting the tissue dissociation with trypsin. The most efficient approach is to dissect as many batches of flies as possible within these 2 hr, then start the trypsin digest for these batches. If more midguts are needed, they can be dissected during the incubation times of the trypsin digest.
Although trypsin is a very potent enzyme and could have detrimental effects on cells, we still obtained enough living, healthy cells for subsequent FAC sorting. The key step of our procedure that allows for the isolation of intact cells is that the dissociated cells are removed from the trypsin solution every 30 min. If the dissected midguts are incubated for 2 &#189; hr in a trypsin containing solution at room temperature, we observed a 20&#8211;30% increase in dead, Sytox-positive cells. It should be pointed out that the trypsin solution we use contains EDTA. The presence of EDTA probably facilitates tissue disintegration by chelating calcium and magnesium ions needed for the proper function of extracellular matrix molecules.
The most crucial steps to successfully sort ISCs from young and old guts are the appropriate initial settings of the FACS and gating parameters using the described controls and following a specific sorting hierarchy. We performed the FAC sorting on an ARIA II Flow Cytometer (FACSDiva software). It is important that the instrument is turned on at least one hour prior to sorting to warm up the lasers. Of note, when FAC sorting of ISCs is performed for the first time, the parameters for sorting and for compensation need to be set using the aforementioned controls: (1) dissociated cells from wild type (e.g. w1118) Drosophila midguts without addition of Sytox &#8212; setting this parameter (Step 4.4.1) prevents sorting cells based on their autofluorescence; (2) dissociated cells from wild type (e.g. w1118) Drosophila midguts with Sytox added &#8212; setting this parameter (Step 4.4.2) allows separating dead from living cells (dead cells have a high autofluorescence and can contaminate the sorted GFP-positive cells); (3) dissociated cells from midguts of the esg-Gal4, UAS-GFP fly line without Sytox &#8212; setting this parameter (Step 4.4.3) ensures that all GFP-positive cells are plotted within the scatter plot. If these parameters are not set properly, the sorted cell population will most likely contain dead cells and debris (Figure 5B, C), many GFP-positive cells will be missed (Figure 5D) and the two distinct peaks for GFP-positive cells as seen in the histogram plot (Figure 2E and Figure 3E) will not be detected. Once the FACS and gating parameters have been set, the instrument is calibrated and ready to sort cells from the esg-GAL4, UAS-GFP fly line. Since these parameters can be saved, all future sorting sessions for ISCs and EBs from the esg-GAL4, UAS-GFP fly line can start from Step 4.5. Although choosing the &#8220;Purity&#8221; mode and performing a two-way purity sort decreases the number of cells sorted, it allows for a higher sorting stringency (Step 4.6 and Figure 4B, C). Of note, the advantage of using Sytox instead of propidium iodide to label dead cells is that there is only a low spillover into the FITC (GFP) channel, which makes it easy to compensate for the spillover.
Our method of enriching for ISCs and EBs, respectively, is based on sorting the cells according to different GFP expression levels. It may be that during aging the misdifferentiated EBs also express GFP at a lower level and could be mistaken as ISCs. However, since the sorted cells also differ in size and granularity, we believe that our sorting strategy is the most suitable to this date to enrich for ISCs and EBs. Also, it is known that cells in an aging midgut retaining ISC identity have a small nucleus15. To obtain more clarity on the identity of the sorted cells, one could sort cells from a transgenic fly line that carries esg-GAL4, UAS-GFP and a Notch signaling reporter transgene. Since Notch has been shown to be active only in the EBs12,13, ISCs isolated from a young midgut would be negative for the Notch reporter, whereas the EBs would be positive for the Notch reporter. However, during aging Notch signaling becomes aberrant in the midgut tissue. Therefore, it needs to be tested whether this experimental set up is indeed more reliable to distinguish between ISCs and EBs isolated from an old midgut.
We have already employed this approach for comparative transcriptome analysis of ISCs from young and old midguts and identified a number of factors that are differentially regulated during aging (unpub. observ.). Additionally, this method allows for analyzing differences in gene expression between ISCs and the EBs. Such investigations will provide insight into the initial molecular changes that occur as a cell enters the differentiation process. Also, the isolation of EBs during aging and subsequent analyses will shed light on the molecular changes of age-induced misdifferentiation. Furthermore, this method can be combined with other genetic tools used in Drosophila to study gene function. In summary, this method offers an unbiased approach to investigate molecular characteristics and changes of ISCs and EBs during aging. This is a valuable tool that will facilitate exploration of aging mechanisms in adult stem and progenitor cells.

An unavoidable consequence of growing old is the decreasing ability of tissues and organs to remain functional. Adult stem cells are essential for maintaining tissue homeostasis and organ functionality, however as organisms age, the stem cells also experience a decline in their biological behavior. This is particularly detrimental to tissues that have a high turnover rate, such as the intestinal epithelium. Hallmarks of aged stem cells include genomic damage, impaired repair mechanisms, impaired cell cycle regulation and misregulated signaling pathways, all of which affect normal stem cell behavior (reviewed in1-3). By manipulating specific signaling pathways or knocking down specific genes, we have gained insight into their roles in regulating and maintaining normal stem cell behavior. Since most of these experiments are candidate molecule approaches, we have very little knowledge about the endogenous molecular changes that occur in stem cells during aging. One way to approach this question is to compare the transcriptome of young versus old stem cells to identify molecules whose expression profile changes significantly during aging. Unfortunately, biological and technical challenges have hampered our progress regarding this approach so far.
Drosophila melanogaster is a highly suitable model organism to study aging since it has a short lifespan (about 60&#8211;70 days) and exhibits aging phenotypes (reviewed in4). Moreover, the aging process in Drosophila can be accelerated by temperature. When keeping the flies at 29 &#176;C, an aged phenotype in the intestinal tissue can already be observed after 15 days5. Furthermore, Drosophila is amenable for a plethora of genetic manipulations. In particular, the Drosophila midgut has emerged as an excellent model system to study the influence of different signaling pathways and environmental challenges on the biology of intestinal stem cells (ISCs) during aging (reviewed in6-10). The Drosophila intestinal epithelium has a high turnover rate and is renewed every two weeks in females and about once a month in males11. ISCs residing in the Drosophila midgut have the capacity to divide and produce a self-renewed ISC and a post-mitotic progenitor cell called the enteroblast (EB)12,13. The EB differentiates into either an absorptive enterocyte or a secretory enteroendocrine cell. To this date, the only marker combination that unambiguously labels an ISC is the expression of the transcription factor escargot (esg) and the Notch ligand Delta (Dl)14. However, this only holds true for a young and healthy gut. During aging, the midgut epithelium is characterized by an increase in ISC proliferation15-17. Additionally, aberrant Notch signaling disrupts the fate decision of ISC daughter cells and induces misdifferentiation of EBs15. This results in an accumulation of cells that are active for Notch signaling and co-express esg and Dl, thereby rendering Dl expression insufficient to identify bona fide stem cells in an aged midgut. The difficulty in identifying true ISCs has impeded the ability to examine endogenous changes in aging ISCs until now.
We have tackled this issue by taking advantage of the esg-Gal4, UAS-GFP transgenic fly line in which the level of GFP expression in ISCs and EBs is inherently different and remains different throughout aging. A similar approach has been described for the isolation of larval neuroblasts and neurons18,19. Midguts of young and old esg-Gal4, UAS-GFP flies were dissected and dissociated into single cells. The cells were then sorted for GFP-positive cells using fluorescence activated cell sorting (FACS). Interestingly, the sorted GFP-positive cells distributed into two distinct peaks based on GFP fluorescence intensity (GFPhigh and GFPlow). Moreover, the distribution of the GFP-positive cells in the two peaks also correlated with cell size: the cells that exhibited low GFP intensity were small and less granular whereas cells with high GFP intensity were larger and more granular. This observation suggested that the smaller ISCs could be distinguished from the larger EBs using FACS based on GFP intensity and choosing appropriate forward scatter (FSC) and side scatter (SSC) settings. Intriguingly, the two peaks remained distinctly separated during aging. Moreover, the ratio of the two peaks changed in a way that reflects the aforementioned hallmarks of aging midguts: namely that the number of large, misdifferentiated EBs increases over time. From these findings we conclude that by sorting for GFP-positive cells using the appropriate FACS parameter settings we can enrich for ISCs and EBs at any time point during aging.
In summary, we introduce a FACS strategy that enables researchers to enrich for two different cell populations, ISCs and EBs, from Drosophila midguts of any age and isolate these cells for further analysis, such as next generation sequencing. This powerful method allows for studying the endogenous molecular mechanisms that are inherent to aging in an enriched population of stem or progenitor cells. The data obtained from these studies will undoubtedly facilitate the identification of conserved molecules that are significant in aging across species.

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			<td height="42" style="height:42px;width:271px;">Forceps: Dumont, Inox Biologie #5</td>
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			<td height="42" style="height:42px;width:271px;">SefarNitex 03-150um/38 (35 &#181;m nylon mesh)</td>
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			<td height="42" style="height:42px;width:271px;">Falcon 5ml Round Bottom Polystyrene Test Tube with Cell Strainer Snap Cap</td>
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			<td height="21" style="height:21px;width:271px;">Polymax 1040</td>
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			<td height="21" style="height:21px;width:271px;">0.5% Trypsin-EDTA</td>
			<td style="width:105px;">Invitrogen</td>
			<td style="width:104px;">15400-054</td>
			<td>Trypsin obtained from a different company most likely has a different activity and the duration of the trypsin digest has to be adjusted accordingly.</td>
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			<td height="42" style="height:42px;width:271px;">SYTOX Blue Dead Cell Stain for flow cytometry</td>
			<td style="width:105px;">Life Technologies</td>
			<td style="width:104px;">S34857</td>
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			<td height="42" style="height:42px;width:271px;">RNAlater Stabilization Solution</td>
			<td style="width:105px;">Life Technologies</td>
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			<td>&#160;other solutions, e.g. Trizol can be used for subsequent RNA isolation</td>
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			<td height="42" style="height:42px;width:271px;">FACSAria II cell sorter</td>
			<td style="width:105px;">Becton Dickinson</td>
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			<td>Turn on one hour prior to sorting</td>
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isolating intestinal stem cells from adult drosophila midguts by facs to study stem cell behavior during aging

Aging tissue is characterized by a continuous decline in functional ability. Adult stem cells are crucial in maintaining tissue homeostasis particularly in tissues that have a high turnover rate such as the intestinal epithelium. However, adult stem cells are also subject to aging processes and the concomitant decline in function. The Drosophila midgut has emerged as an ideal model system to study molecular mechanisms that interfere with the intestinal stem cells&#8217; (ISCs) ability to function in tissue homeostasis. Although adult ISCs can be easily identified and isolated from midguts of young flies, it has been a major challenge to study endogenous molecular changes of ISCs during aging. This is due to the lack of a combination of molecular markers suitable to isolate ISCs from aged intestines. Here we propose a method that allows for successful dissociation of midgut tissue into living cells that can subsequently be separated into distinct populations by FACS. By using dissociated cells from the esg-Gal4, UAS-GFP fly line, in which both ISCs and the enteroblast (EB) progenitor cells express GFP, two populations of cells are distinguished based on different GFP intensities. These differences in GFP expression correlate with differences in cell size and granularity and represent enriched populations of ISCs and EBs. Intriguingly, the two GFP-positive cell populations remain distinctly separated during aging, presenting a novel technique for identifying and isolating cell populations enriched for either ISCs or EBs at any time point during aging. The further analysis, for example transcriptome analysis, of these particular cell populations at various time points during aging is now possible and this will facilitate the examination of endogenous molecular changes that occur in these cells during aging.

To obtain between 50,000&#8211;100,000 cells from FAC sorting, between 160 and 200 midguts need to be dissected. Obviously this is the most time consuming step of the whole procedure. The cartoon shown in Figure 1A illustrates the major steps of gut dissection, which are described in detail in the protocol provided here. This procedure can be individually modified. A dissected, whole gastrointestinal tract is shown in Figure 1B.
When all of the midgut tissue has been digested, immediately continue with FAC sorting. Following the gating strategy described in the protocol allows for the successful identification and sorting of a cell population enriched for ISCs and for EBs from young (Figure 2) and from old midguts (Figure 3). The P1 gate is set to include only healthy living cells and to gate out dead cells. Cells that plot above 103 on the logarithmic y-axis when using the Pacific Blue channel are defined as dead cells. The dots that plot below 40 on the x-axis (FSC-A) are mostly debris and therefore are also excluded (Figure 2A). In the scatter plot of SSC-A vs. FSC-A the cells are distributed based on their size and granularity. For an optimal resolution, the cells are placed in the scatter plot as shown in Figure 2B by adjusting the photomultiplier tube (PMT) voltage. In the scatter plots FSC-H vs. FSC-W and SSC-H vs. SSC-W single cells are separated from aggregates and doublets based on size (Figure 2C) and based on granularity (Figure 2D). When depicting the cells included in gate P4 in a histogram plot, the distinct separation of GFP-negative, GFPlow (gate P5) and GFPhigh (gate P6) cells is visible (Figure 2E). Cells exhibiting lower GFP intensity are small and less granular and represent ISCs. Cells exhibiting higher GFP intensity are larger and more granular and represent EBs. Reverse Transcriptase (RT)-PCR for Dl on cDNA synthesized from RNA of cells of each GFP-positive population (gates P5, P6) revealed that the Dl signal is indeed stronger in the smaller, GFPlow cells than in the larger, GFPhigh cells (Figure 2H). The cells were then backgated and depicted in contour plots to confirm that the GFPlow (gate P5) and GFPhigh (gate P6) cells differ in size and granularity (Figure 2F) and are still alive (Figure 2G). Of note, the two peaks of GFP-positive cells (GFPlow and GFPhigh) can only be nicely distinguished if the FITC (GFP) channel has been calibrated properly using the controls described in the protocol.
The same gating strategy was used when sorting ISCs derived from old guts (Figure 3). The scatter plots (Figure 3A-D), the histogram (Figure 3E) and the contour plots (Figure 3F, G) are analogous to the ones shown in Figure 2. As mentioned above, there is no bona fide marker to identify ISCs in old midguts and therefore no RT-PCR data is presented here. However, the intriguing observation here is that the two peaks containing GFPlow (gate P5) or GFPhigh (gate P6) cells remain distinctly separated during aging. Furthermore, the number of cells in the GFPhigh (gate P6) peak significantly increases during aging, which clearly emulates the known accumulation of misdifferentiated EBs with age. The change in the ratio of the two cell populations can also be seen in the scatter plots (compare Figure 3A-D with Figure 2A-D) and in the contour plots (compare Figure 3F, G with Figure 2F, G). From these findings we conclude that by sorting for GFP-positive cells using FACS we can enrich for ISCs and EBs in young and old midguts.
To validate the purity of the isolated ISCs and EBs, a post sort analysis was performed (Figure 4). The histogram plots of the post-sorted ISCs and EBs (Figure 4B, C) depict purities between 95% and 98%.
If the hierarchy of setting the FACS parameters as described above is strictly followed, the two different cell populations (GFPlow, small and GFPhigh, larger) can already be distinguished in a scatter plot GFP vs. FSC-A (Figure 5A). These two cell populations cannot be distinguished if this hierarchy is disregarded (Figure 5B-D).
<img alt="Figure 1" src="/files/ftp_upload/52223/52223fig1highres.jpg" /> 
Figure 1: (A) A schematic of the major steps of dissecting the fly intestine. First, the head is removed (removal of the wings is optional) followed by a separation of the thorax and abdomen to expose the gut. The gut is subsequently freed from the body cavity in the following steps. The black arrows show the progression of dissection, whereas the dark red arrows denote the pull direction. The red lines in the last image indicate the anterior and posterior boundaries of the midgut. (B) A light microscope image of the adult fly intestine. The main regions and anatomical features are labeled. Red lines mark the boundaries of the midgut.
<img alt="Figure 2" src="/files/ftp_upload/52223/52223fig2highres.jpg" /> 
Figure 2: FAC sorting strategy to identify and isolate ISCs and EBs from young (7 days) midguts. For better visualization, cells representing ISCs are highlighted in red and cells representing EBs are highlighted in blue in the scatter plots (A-D) and in the contour plots (F,G). (A) The P1 gate is set to exclude dead, Sytox-positive cells plotted above 103 on the logarithmic y-axis. The threshold of the FSC-A is set at 40 to also exclude dead cells and debris. (B) Cells were gated for FSC-A and SSC-A to select cells according to size and granularity (gate P2). The histogram plot (E) was used in parallel to identify the GFP-positive cells in the FSC-A vs. SSC-A scatter plot (B). (C, D) The scatter plots FSC-H vs. FSC-W and SSC-H vs. SSC-W serve to remove aggregates and doublets and select for singlets (gate P3 in C and gate P4 in D). (E) The histogram plot shows the number of cells and their GFP intensity. Two peaks, GFPlow (gate P5) and GFPhigh (gate P6) can be distinguished. (F, G) Cells were back-gated in a contour plot to verify that the two distinct GFP-positive cell populations are of the correct size (F) and contain living cells (G). (H) Reverse Transcriptase (RT)-PCR for Dl on cDNA synthesized from RNA isolated from the cells present in the first peak (gate P5) and in the second peak (gate P6), respectively. More Dl expression could be detected in cells present in gate P5 vs. gate P6. Tubulin served as a loading control. <a href="https://www.jove.com/files/ftp_upload/52223/52223fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/52223/52223fig3highres.jpg" /> 
Figure 3: FAC sorting strategy to identify and isolate ISCs and EBs from old (60 days) midguts. For better visualization, cells representing ISCs are highlighted in red and cells representing EBs are highlighted in blue in the scatter plots (A-D) and in the contour plots (F,G). (A) The P1 gate is set to exclude dead, Sytox-positive cells plotted above 103 on the logarithmic y-axis. The threshold of the FSC-A is set at 40 to also exclude dead cells and debris. Of note, the age-dependent increase in larger GFP-positive cells is already obvious in this plot. (B) Cells were gated for FSC-A and SSC-A to select cells according to size and granularity (gate P2). The histogram plot (E) was used in parallel to identify the GFP-positive cells in the FSC-A vs. SSC-A scatter plot (B). (C, D) The scatter plots FSC-H vs. FSC-W and SSC-H vs. SSC-W serve to remove aggregates and doublets and select for singlets (gate P3 in C and gate P4 in D). (E) The histogram plot shows the number of cells and their GFP intensity. Two peaks, GFPlow (gate P5) and GFPhigh (gate P6) can be distinguished. Of note, the cell population GFPhigh containing larger cells has increased in number during aging. (F, G) Cells were back-gated in a contour plot to verify that the two distinct GFP-positive cell populations are of the correct size (F) and contain living cells (G). <a href="https://www.jove.com/files/ftp_upload/52223/52223fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" src="/files/ftp_upload/52223/52223fig4highres.jpg" /> 
Figure 4: A post sort analysis was performed to determine the purity of the isolated ISCs and EBs. (A) GFP-positive cells from young (7 days) and old (60 days) midguts were FAC sorted and the histogram plots show their distribution into two peaks based on GFP intensity. (B) The post sort analysis demonstrates the purity of the isolated ISCs from young and old midguts which is &#62;97%. (C) The post sort analysis of sorted EBs from young and old midguts shows a purity of &#62;95%. The slight impurities may result from fluorescence quenching or mechanically damaged GFP expressing cells caused by re-sorting the cells. <a href="https://www.jove.com/files/ftp_upload/52223/52223fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" src="/files/ftp_upload/52223/52223fig5highres.jpg" /> 
Figure 5: Examples of scatter plots that show suboptimal FACS data, which is seen when the FACS parameters were not set properly. (A) Representative FACS profile of all cells when the FACS parameters were set properly based on the controls described in the protocol. The cell population containing ISCs is circled in red and the cell population containing EBs is circled in blue. The cells circled in green are dead cells that have a stronger autofluorescence compared to living cells, which are plotted below 103 on the logarithmic y-axis. (B) The scatter plot depicts a typical result obtained when the FACS instrument was not calibrated. No GFP-positive cells are detected. (C) If the FSC is not set properly, the different GFP-positive cell populations are not detected. (D) If the FITC (GFP) channel is not adjusted correctly, the majority of GFP-positive cells to be sorted are not plotted in the scatter plot but rather along the upper edge of the plot. Also, in the plot shown here, the limit for autofluorescence was not adjusted, hence cells that plot above 102 on the logarithmic y-axis are actually autofluorescent and could be mistaken as GFP-positive cells.

Watch this Scientific Journal Video about Isolating Intestinal Stem Cells from Adult Drosophila Midguts by FACS to Study Stem Cell Behavior During Aging at JoVE.com

Isolating Intestinal Stem Cells from Adult Drosophila Midguts by FACS to Study Stem Cell Behavior During Aging

Understanding the endogenous molecular changes in adult stem cells during aging requires isolating the cells of interest. The method described here presents a simple and robust approach to enrich for and isolate Drosophila intestinal stem cells and the enteroblast progenitor cells by FACS at any time point during aging.

Isolating Intestinal Stem Cells from Adult Drosophila Midguts by FACS to Study Stem Cell Behavior During Aging

Aging tissue is characterized by a continuous decline in functional ability. Adult stem cells are crucial in maintaining tissue homeostasis particularly ...

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20.0K Views.  Universität Ulm. Understanding the endogenous molecular changes in adult stem cells during aging requires isolating the cells of interest. The method described here presents a simple and robust approach to enrich for and isolate Drosophila intestinal stem cells and the enteroblast progenitor cells by FACS at any time point during aging. 

Video: Isolating Intestinal Stem Cells from Adult Drosophila Midguts by FACS to Study Stem Cell Behavior During Aging

Transplantation of Whole Kidney Marrow in Adult Zebrafish

Hematopoietic stem cells (HSC) are a rare population of pluripotent cells that maintain all the differentiated blood lineages throughout the life of an organism. The functional definition of a HSC is a transplanted cell that has the ability to reconstitute all the blood lineages of an irradiated recipient long term. This designation was established by decades of seminal work in mammalian systems. Using hematopoietic cell transplantation (HCT) and reverse genetic manipulations in the mouse, the underlying regulatory factors of HSC biology are beginning to be unveiled, but are still largely under-explored. Recently, the zebrafish has emerged as a powerful genetic model to study vertebrate hematopoiesis. Establishing HCT in zebrafish will allow scientists to utilize the large-scale genetic and chemical screening methodologies available in zebrafish to reveal novel mechanisms underlying HSC regulation. In this article, we demonstrate a method to perform HCT in adult zebrafish. We show the dissection and preparation of zebrafish whole kidney marrow, the site of adult hematopoiesis in the zebrafish, and the introduction of these donor cells into the circulation of irradiated recipient fish via intracardiac injection. Additionally, we describe the post-transplant care of fish in an "ICU" to increase their long-term health. In general, gentle care of the fish before, during, and after the transplant is critical to increase the number of fish that will survive more than one month following the procedure, which is essential for assessment of long term (&lt;3 month) engraftment. The experimental data used to establish this protocol will be published elsewhere. The establishment of this protocol will allow for the merger of large-scale zebrafish genetics and transplant biology.

In this article, we demonstrate a method to perform HCT in adult zebrafish.

Hematopoietic stem cells (HSC) are a rare population of pluripotent cells that maintain all the differentiated blood lineages throughout the life of an ...

Derivation of Hematopoietic Stem Cells from Murine Embryonic Stem Cells

A stem cell is defined as a cell with the capacity to both self-renew and generate multiple differentiated progeny.  Embryonic stem cells (ESC) are derived from the blastocyst of the early embryo and are pluripotent in differentiative ability.  Their vast differentiative potential has made them the focus of much research centered on deducing how to coax them to generate clinically useful cell types.  The successful derivation of hematopoietic stem cells (HSC) from mouse ESC has recently been accomplished and can be visualized in this video protocol.  HSC, arguably the most clinically exploited cell population, are used to treat a myriad of hematopoietic malignancies and disorders.  However, many patients that might benefit from HSC therapy lack access to suitable donors.  ESC could provide an alternative source of HSC for these patients.  The following protocol establishes a baseline from which ESC-HSC can be studied and inform efforts to isolate HSC from human ESC.  In this protocol, ESC are differentiated as embryoid bodies (EBs) for 6 days in commercially available serum pre-screened for optimal hematopoietic differentiation.  EBs are then dissociated and infected with retroviral HoxB4.  Infected EB-derived cells are plated on OP9 stroma, a bone marrow stromal cell line derived from the calvaria of  M-CSF-/- mice, and co-cultured in the presence of hematopoiesis promoting cytokines for ten days.  During this co-culture, the infected cells expand greatly, resulting in the generation a heterogeneous pool of 100s of millions of cells.  These cells can then be used to rescue and reconstitute lethally irradiated mice.

This protocol details the derivation of transplantable hematopoietic stem cells from mouse embryonic stem cells (ESC) and their subsequent injection into lethally irradiated recipient mice. Briefly, ESC are differentiated as embryoid bodies, which are then infected with retroviral HoxB4 and co-cultured with OP9 stromal cells and hematopoietic cytokines.

A stem cell is defined as a cell with the capacity to both self-renew and generate multiple differentiated progeny.  Embryonic stem cells (ESC) are ...

Derivation of Human Embryonic Stem Cells by Immunosurgery

The ability of human embryonic stem cells to self-renew and differentiate into all cell types of 
the body suggests that they hold great promise for both medical applications and as a research 
tool for addressing fundamental questions in development and disease. Here, we provide a 
concise, step-by-step protocol for the derivation of human embryonic stem cells from embryos 
by immunosurgical isolation of the inner cell mass. 


The ability of human embryonic stem cells to self-renew and differentiate into all cell types of 
the body suggests that they hold great promise for both medical applications and as a research 
tool for addressing fundamental questions in development and disease. Here, we provide a 
concise, step-by-step protocol for the derivation of human embryonic stem cells from embryos 
by immunosurgical isolation of the inner cell mass.

The ability of human embryonic stem cells to self-renew and differentiate into all cell types of 
the body suggests that they hold great promise for both ...

Isolation and Large Scale Expansion of Adult Human Endothelial Colony Forming Progenitor Cells

This paper introduces a novel recovery strategy for endothelial colony forming progenitor cells (ECFCs) from heparinized but otherwise unmanipulated adult human peripheral blood within a mean of 12 days. After large scale expansion &gt;1x108 ECFCs can be obtained for further tests. Advantageously by using pHPL the contact of human cells with bovine serum antigens can be excluded. By flow cytometry and immunohistochemistry the isolated cells can be characterized as ECFC and their in vitro functionality to form vascular like structures can be tested in a matrigel assay. Further these cells can be subcutaneously injected in a mouse model to form functional, perfused vessels in vivo. After long term expansion and cryopreservation proliferation, function and genomic stability appear to be preserved. 3,4
This animal-protein free isolation and expansion method is easily applicable to generate a large quantity of ECFCs.

Endothelial colony forming progenitor cells (ECFCs) are a promising tool to study vascular homeostasis and repair.1,2 This paper introduces a novel animal-serum free method for isolation and expansion of ECFC from heparinised adult human peripheral blood with pooled human platelet lysate (pHPL) diminishing the risk of anti-bovine immunisation.

This paper introduces a novel recovery strategy for endothelial colony forming progenitor cells (ECFCs) from heparinized but otherwise unmanipulated adult ...

Isolation and Animal Serum Free Expansion of Human Umbilical Cord Derived Mesenchymal Stromal Cells (MSCs) and Endothelial Colony Forming Progenitor Cells (ECFCs)

The umbilical cord is a rich source for progenitor cells with high proliferative potential including mesenchymal stromal cells (also termed mesenchymal stem cells, MSCs) and endothelial colony forming progenitor cells (ECFCs). Both cell types are key players in maintaining the integrity of tissue and are probably also involved in regenerative processes and tumor formation.
To study their biology and function in a comparative manner it is important to have both cells types available from the same donor. It may also be beneficial for regenerative purposes to derive MSCs and ECFCs from the same tissue.
Because cellular therapeutics should eventually find their way from bench to bedside we established a new method to isolate and further expand progenitor cells without the use of animal protein. Pooled human platelet lysate (pHPL) replaced fetal bovine serum in all steps of our protocol to completely avoid contact of the cells to xenogeneic proteins.
This video demonstrates a methodology for the isolation and expansion of progenitor cells from one umbilical cord.
All materials and procedures will be described.

Isolation and Animal Serum Free Expansion of Human Umbilical Cord Derived Mesenchymal Stromal Cells MSCs and Endothelial Colony Forming Progenitor Cells ECFCs

This protocol describes the isolation and subsequent expansion of mesenchymal stromal cells and endothelial colony forming cells without the use of animal serum to generate autologous pairs for experimental transplantation purposes.

The umbilical cord is a rich source for progenitor cells with high proliferative potential including mesenchymal stromal cells (also termed mesenchymal ...

Isolating Stem Cells from Soft Musculoskeletal Tissues

Adult stem cells have long been discussed in regards to their application in regenerative medicine. Adult stem cells have generated a great deal of excitement for treating injured and diseased tissues due to their impressive capabilities to undergo multi-lineage cell differentiation and their self-renewal ability. Most importantly, these qualities have made them advantageous for use in autologous cell transplantation therapies. The current protocol will introduce the readers to the modified preplate technique where soft tissues of the musculoskeletal system, e.g. tendon and muscle, are 1st enzymatically dissociated and then placed in collagen coated flasks with medium. The supernatant, which is composed of medium and the remaining floating cells, is serially transferred daily to new flasks. The stem cells are the slowest to adhere to the flasks which is usually takes 5-7 days (serial transfers or preplates) . By using this technique, adult stem cells present in these tissues can be easily harvested through fairly non-invasive procedures.

Isolating adult stem cells from musculoskeletal soft tissues based on the cell's adherence speed to flask.

Adult stem cells have long been discussed in regards to their application in regenerative medicine. Adult stem cells have generated a great deal of ...

Fate Mapping of Human Embryonic Stem Cells by Teratoma Formation 

Human embryonic stem cells (hESCs) have an unlimited capacity for self-renewal, and the ability to differentiate into cells derived from all three embryonic germ layers (1). Directed differentiation of hESCs into specific cell types has generated much interest in the field of regenerative medicine (e.g., (2-5)), and methods for determining the in vivo fate of selected or manipulated hESCs are essential to this endeavor. We have adapted a highly efficient teratoma formation assay for this purpose. A small number of specifically selected hESCs is mixed with undifferentiated wild type hESCs and Phaseolus vulgaris lectin to form a cell pellet. This is grafted beneath the kidney capsule in an immunodeficient mouse. As few as 2.5 x 105 hESCs are needed to form a 16 cm3 teratoma within 8-12 weeks. The fate of the originally selected hESCs can then be determined by immunohistochemistry. This method provides a valuable tool for characterizing tissue-specific reagents for cell-based therapy.

Fate Mapping of Human Embryonic Stem Cells by Teratoma Formation

Directed differentiation of hESCs into specific cells has generated much interest in regenerative medicine. We provide a concise, step-by-step protocol for determining the in vivo fate of selected hESCs that provides a valuable tool for characterizing tissue-specific reagents for cell-based therapy.

Human embryonic stem cells (hESCs) have an unlimited capacity for self-renewal, and the ability to differentiate into cells derived from all three ...

Lentiviral-mediated Knockdown During Ex Vivo Erythropoiesis of Human Hematopoietic Stem Cells

Erythropoiesis is a commonly used model system to study cell differentiation. During erythropoiesis, pluripotent adult human hematopoietic stem cells (HSCs) differentiate into oligopotent progenitors, committed precursors and mature red blood cells 1. This process is regulated for a large part at the level of gene expression, whereby specific transcription factors activate lineage-specific genes while concomitantly repressing genes that are specific to other cell types 2. Studies on transcription factors regulating erythropoiesis are often performed using human and murine cell lines that represent, to some extent, erythroid cells at given stages of differentiation 3-5. However transformed cell lines can only partially mimic erythroid cells and most importantly they do not allow one to comprehensibly study the dynamic changes that occur as cells progress through many stages towards their final erythroid fate. Therefore, a current challenge remains the development of a protocol to obtain relatively homogenous populations of primary HSCs and erythroid cells at various stages of differentiation in quantities that are sufficient to perform genomics and proteomics experiments.
Here we describe an ex vivo cell culture protocol to induce erythroid differentiation from human hematopoietic stem/progenitor cells that have been isolated from either cord blood, bone marrow, or adult peripheral blood mobilized with G-CSF (leukapheresis). This culture system, initially developed by the Douay laboratory 6, uses cytokines and co-culture on mesenchymal cells to mimic the bone marrow microenvironment. Using this ex vivo differentiation protocol, we observe a strong amplification of erythroid progenitors, an induction of differentiation exclusively towards the erythroid lineage and a complete maturation to the stage of enucleated red blood cells. Thus, this system provides an opportunity to study the molecular mechanism of transcriptional regulation as hematopoietic stem cells progress along the erythroid lineage. 
Studying erythropoiesis at the transcriptional level also requires the ability to over-express or knockdown specific factors in primary erythroid cells. For this purpose, we use a lentivirus-mediated gene delivery system that allows for the efficient infection of both dividing and non-dividing cells 7. Here we show that we are able to efficiently knockdown the transcription factor TAL1 in primary human erythroid cells. In addition, GFP expression demonstrates an efficiency of lentiviral infection close to 90%. Thus, our protocol provides a highly useful system for characterization of the regulatory network of transcription factors that control erythropoiesis.

Lentiviral-mediated Knockdown During Ex Vivo Erythropoiesis of Human Hematopoietic Stem Cells

An ex vivo protocol to generate mature human red blood cells from hematopoietic stem/progenitors is described. Additionally we describe an efficient lentiviral-delivery method to knockdown the transcription factor TAL1 in primary erythroid cells. The efficiency of lentivirus mediated gene delivery is demonstrated using GFP expressing viruses.

Erythropoiesis is a commonly used model system to study cell differentiation. During erythropoiesis, pluripotent adult human hematopoietic stem cells ...

Selecting and Isolating Colonies of Human Induced Pluripotent Stem Cells Reprogrammed from Adult Fibroblasts

Herein we present a protocol of reprogramming human adult fibroblasts into human induced pluripotent stem cells (hiPSC) using retroviral vectors encoding Oct3/4, Sox2, Klf4 and c-myc (OSKM) in the presence of sodium butyrate 1-3. We used this method to reprogram late passage (&gt;p10) human adult fibroblasts derived from Friedreich's ataxia patient (GM03665, Coriell Repository). The reprogramming approach includes highly efficient transduction protocol using repetitive centrifugation of fibroblasts in the presence of virus-containing media. The reprogrammed hiPSC colonies were identified using live immunostaining for Tra-1-81, a surface marker of pluripotent cells, separated from non-reprogrammed fibroblasts and manually passaged 4,5. These hiPSC were then transferred to Matrigel plates and grown in feeder-free conditions, directly from the reprogramming plate. Starting from the first passage, hiPSC colonies demonstrate characteristic hES-like morphology. Using this protocol more than 70% of selected colonies can be successfully expanded and established into cell lines. The established hiPSC lines displayed characteristic pluripotency markers including surface markers TRA-1-60 and SSEA-4, as well as nuclear markers Oct3/4, Sox2 and Nanog. 
The protocol presented here has been established and tested using adult fibroblasts obtained from Friedreich's ataxia patients and control individuals 6, human newborn fibroblasts, as well as human keratinocytes.

We present a protocol for efficient reprogramming of human somatic cells into human induced pluripotent stem cells (hiPSC) using retroviral vectors encoding Oct3/4, Sox2, Klf4 and c-myc (OSKM) and identification of correctly reprogrammed hiPSC by live staining with Tra-1-81 antibody.

Herein we present a protocol of reprogramming human adult fibroblasts into human induced pluripotent stem cells (hiPSC) using retroviral vectors encoding ...

Isolation and Culture of Individual Myofibers and their Satellite Cells from Adult Skeletal Muscle

Muscle regeneration in the adult is performed by resident stem cells called satellite cells. Satellite cells are defined by their position between the basal lamina and the sarcolemma of each myofiber. Current knowledge of their behavior heavily relies on the use of the single myofiber isolation protocol. In 1985, Bischoff described a protocol to isolate single live fibers from the Flexor Digitorum Brevis (FDB) of adult rats with the goal to create an in vitro system in which the physical association between the myofiber and its stem cells is preserved 1. In 1995, Rosenblattmodified the Bischoff protocol such that myofibers are singly picked and handled separately after collagenase digestion instead of being isolated by gravity sedimentation 2, 3. The Rosenblatt or Bischoff protocol has since been adapted to different muscles, age or conditions 3-6. The single myofiber isolation technique is an indispensable tool due its unique advantages. First, in the single myofiber protocol, satellite cells are maintained beneath the basal lamina. This is a unique feature of the protocol as other techniques such as Fluorescence Activated Cell Sorting require chemical and mechanical tissue dissociation 7. Although the myofiber culture system cannot substitute for in vivo studies, it does offer an excellent platform to address relevant biological properties of muscle stem cells. Single myofibers can be cultured in standard plating conditions or in floating conditions. Satellite cells on floating myofibers are subjected to virtually no other influence than the myofiber environment. Substrate stiffness and coating have been shown to influence satellite cells' ability to regenerate muscles 8, 9 so being able to control each of these factors independently allows discrimination between niche-dependent and -independent responses. Different concentrations of serum have also been shown to have an effect on the transition from quiescence to activation. To preserve the quiescence state of its associated satellite cells, fibers should be kept in low serum medium 1-3. This is particularly useful when studying genes involved in the quiescence state. In serum rich medium, satellite cells quickly activate, proliferate, migrate and differentiate, thus mimicking the in vivo regenerative process 1-3. The system can be used to perform a variety of assays such as the testing of chemical inhibitors; ectopic expression of genes by virus delivery; oligonucleotide based gene knock-down or live imaging. This video article describes the protocol currently used in our laboratory to isolate single myofibers from the Extensor Digitorum Longus (EDL) muscle of adult mice (6-8 weeks old).

Isolation and culture of myofibers is the gold standard in vitro system to study the transition of satellite cells through quiescence, activation and differentiation. Importantly, the single myofiber culture system preserves the myofiber/stem cell association, which is an essential component of the muscle stem cell niche.

Muscle  regeneration in the adult is performed by resident stem cells called satellite  cells. Satellite cells are defined by  their position between the ...

Isolating Intestinal Stem Cells from Adult Drosophila Midguts by FACS to Study Stem Cell Behavior During Aging

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Lentiviral-mediated Knockdown During Ex Vivo Erythropoiesis of Human Hematopoietic Stem Cells

Selecting and Isolating Colonies of Human Induced Pluripotent Stem Cells Reprogrammed from Adult Fibroblasts

Isolation and Culture of Individual Myofibers and their Satellite Cells from Adult Skeletal Muscle