Name: isolating intestinal stem cells from adult drosophila midguts by facs to study stem cell behavior during aging
Uploaded: 2014-12-16T15:00:00.000+00:00
Duration: 10 min 57 s
Description: 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

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.

<table><tbody><tr><td>Forceps: Dumont, Inox Biologie #5</td><td>Fine Science Tools</td><td>11252-20</td><td></td></tr><tr><td>SefarNitex 03-150um/38 (35 &amp;micro;m nylon mesh)</td><td>Sefar</td><td>3A03-0150-102-00</td><td></td></tr><tr><td>Falcon 5 ml Round Bottom Polystyrene Test Tube with Cell Strainer Snap Cap</td><td>Corning</td><td>352235</td><td></td></tr><tr><td>Polymax 1040</td><td>Heidolph</td><td>543-42210-00</td><td></td></tr><tr><td>Albumin from bovine serum (BSA)</td><td>Sigma</td><td>A4503-50G</td><td></td></tr><tr><td>0.5% Trypsin-EDTA</td><td>Invitrogen</td><td>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></tr><tr><td>SYTOX Blue Dead Cell Stain for flow cytometry</td><td>Life Technologies</td><td>S34857</td><td></td></tr><tr><td>RNAlater Stabilization Solution</td><td>Life Technologies</td><td>AM7023</td><td>Other solutions, &lt;em&gt;e.g.&lt;/em&gt;, Trizol can be used for subsequent RNA isolation</td></tr><tr><td>FACSAria II cell sorter</td><td>Becton Dickinson</td><td></td><td>Turn on one hour prior to sorting</td></tr></tbody></table>

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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Research

JoVE Journal

Biology

20.1K 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

The Drosophila Imaginal Disc Tumor Model: Visualization and Quantification of Gene Expression and Tumor Invasiveness Using Genetic Mosaics

Drosophila melanogaster has emerged as a powerful experimental system for functional and mechanistic studies of tumor development and progression in the context of a whole organism. Sophisticated techniques to generate genetic mosaics facilitate induction of visually marked, genetically defined clones surrounded by normal tissue. The clones can be analyzed through diverse molecular, cellular and omics approaches. This study describes how to generate fluorescently labeled clonal tumors of varying malignancy in the eye/antennal imaginal discs (EAD) of Drosophila larvae using the Mosaic Analysis with a Repressible Cell Marker (MARCM) technique. It describes procedures how to recover the mosaic EAD and brain from the larvae and how to process them for simultaneous imaging of fluorescent transgenic reporters and antibody staining. To facilitate molecular characterization of the mosaic tissue, we describe a protocol for isolation of total RNA from the EAD. The dissection procedure is suitable to recover EAD and brains from any larval stage. The fixation and staining protocol for imaginal discs works with a number of transgenic reporters and antibodies that recognize Drosophila proteins. The protocol for RNA isolation can be applied to various larval organs, whole larvae, and adult flies. Total RNA can be used for profiling of gene expression changes using candidate or genome-wide approaches. Finally, we detail a method for quantifying invasiveness of the clonal tumors. Although this method has limited use, its underlying concept is broadly applicable to other quantitative studies where cognitive bias must be avoided.

The Drosophila Imaginal Disc Tumor Model: Visualization and Quantification of Gene Expression and Tumor Invasiveness Using Genetic Mosaics

This protocol demonstrates how to generate fluorescently marked, genetically defined clonal tumors in the Drosophila eye/antennal imaginal discs (EAD). It describes how to dissect the EAD and brain from the third instar larvae and how to process them to visualize and quantify gene expression changes and tumor invasiveness.

Drosophila melanogaster has emerged as a powerful experimental system for functional and mechanistic studies of tumor development and progression in the ...

Cancer Research

A FACS-based Protocol to Isolate RNA from the Secondary Cells of Drosophila Male Accessory Glands

To understand the function of an organ, it is often useful to understand the role of its constituent cell populations. Unfortunately, the rarity of individual cell populations often makes it difficult to obtain enough material for molecular studies. For example, the accessory gland of the Drosophila male reproductive system contains two distinct secretory cell types. The main cells make up 96% of the secretory cells of the gland, while the secondary cells (SC) make up the remaining 4% of cells (about 80 cells per male). Although both cell types produce important components of the seminal fluid, only a few genes are known to be specific to the SCs. The rarity of SCs has, thus far, hindered transcriptomic analysis study of this important cell type. Here, a method is presented that allows for the purification of SCs for RNA extraction and sequencing. The protocol consists in first dissecting glands from flies expressing a SC-specific GFP reporter and then subjecting these glands to protease digestion and mechanical dissociation to obtain individual cells. Following these steps, individual, living, GFP-marked cells are sorted using a fluorescent activated cell sorter (FACS) for RNA purification. This procedure yields SC-specific RNAs from ~40 males per condition for downstream RT-qPCR and/or RNA sequencing in the course of one day. The rapidity and simplicity of the procedure allows for the transcriptomes of many different flies, from different genotypes or environmental conditions, to be determined in a short period of time.

A FACS-based Protocol to Isolate RNA from the Secondary Cells of Drosophila Male Accessory Glands

Here, we present a protocol to dissociate and sort a specific cell population from the Drosophila male accessory glands (secondary cells) for RNA sequencing and RT-qPCR. Cell isolation is accomplished through FACS purification of GFP-expressing secondary cells after a multistep-dissociation process requiring dissection, proteases digestion and mechanical dispersion.

To understand the function of an organ, it is often useful to understand the role of its constituent cell populations. Unfortunately, the rarity of ...

Genetics

Methods for Imaging Intracellular pH of the Follicle Stem Cell Lineage in Live Drosophila Ovarian Tissue

Changes in intracellular pH (pHi) play important roles in the regulation of many cellular functions, including metabolism, proliferation, and differentiation. Typically, pHi dynamics are determined in cultured cells, which are amenable to measuring and experimentally manipulating pHi. However, the recent development of new tools and methodologies has made it possible to study pHi dynamics within intact, live tissue. For Drosophila research, one important development was the generation of a transgenic line carrying a pHi biosensor, mCherry::pHluorin. Here, we describe a protocol that we routinely use for imaging live Drosophila ovarioles to measure pHi in the epithelial follicle stem cell (FSC) lineage in mCherry::pHluorin transgenic wild type lines; however, the methods described here can be easily adapted for other tissues, including the wing discs and eye epithelium. We describe techniques for expressing mCherry::pHluorin in the FSC lineage, maintaining ovarian tissue during live imaging, and acquiring and analyzing images to obtain pHi values.

Methods for Imaging Intracellular pH of the Follicle Stem Cell Lineage in Live Drosophila Ovarian Tissue

We provide a protocol for imaging intracellular pH of an epithelial stem cell lineage in live Drosophila ovarian tissue. We describe methods to generate transgenic flies expressing a pH biosensor, mCherry::pHluorin, image the biosensor using quantitative fluorescence imaging, generate standard curves, and convert fluorescence intensity values to pH values.

Changes in intracellular pH (pHi) play important roles in the regulation of many cellular functions, including metabolism, proliferation, and ...

Developmental Biology

Dissection and Staining of Drosophila Pupal Ovaries

Unlike adult Drosophila ovaries, pupal ovaries are relatively difficult to access and examine due to their small size, translucence, and encasing within a pupal case. The challenge of dissecting pupal ovaries also lies in their physical location within the pupa: the ovaries are surrounded by fat body cells inside the pupal abdomen, and these fat cells must be removed to allow for proper antibody staining. To overcome these challenges, this protocol utilizes customized Pasteur pipets to extract fat body cells from the pupal abdomen. Moreover, a chambered coverglass is used in place of a microcentrifuge tube during the staining process to improve visibility of the pupae. However, despite these and other advantages of the tools used in this protocol, successful execution of these techniques may still involve several days of practice due to the small size of pupal ovaries. The techniques outlined in this protocol could be applied to time course experiments in which ovaries are analyzed at various stages of pupal development.

Dissection and Staining of Drosophila Pupal Ovaries

The Drosophila ovary is an excellent model system for studying stem cell niche development. Though methods for dissecting larval and adult ovaries have been published, pupal ovary dissections require different techniques that have not been published in detail. Here we outline a protocol for dissecting, staining, and mounting pupal ovaries.

Unlike adult Drosophila ovaries, pupal ovaries are relatively difficult to access and examine due to their small size, translucence, and encasing within a ...

Dissection and Live-Imaging of the Late Embryonic Drosophila Gonad

The Drosophila melanogaster male embryonic gonad is an advantageous model to study various aspects of developmental biology including, but not limited to, germ cell development, piRNA biology, and niche formation. Here, we present a dissection technique to live-image the gonad ex vivo during a period when in vivo live-imaging is highly ineffective. This protocol outlines how to transfer embryos to an imaging dish, choose appropriately-staged male embryos, and dissect the gonad from its surrounding tissue while still maintaining its structural integrity. Following dissection, gonads can be imaged using a confocal microscope to visualize dynamic cellular processes. The dissection procedure requires precise timing and dexterity, but we provide insight on how to prevent common mistakes and how to overcome these challenges. To our knowledge this is the first dissection protocol for the Drosophila embryonic gonad, and will permit live-imaging during an otherwise inaccessible window of time. This technique can be combined with pharmacological or cell-type specific transgenic manipulations to study any dynamic processes occurring within or between the&#160;cells in their natural gonadal environment.

Dissection and Live-Imaging of the Late Embryonic Drosophila Gonad

Here, we provide a dissection protocol required to live-image the late embryonic Drosophila male gonad. This protocol will permit observation of dynamic cellular processes under normal conditions or after transgenic or pharmacological manipulation.

The Drosophila melanogaster male embryonic gonad is an advantageous model to study various aspects of developmental biology including, but not limited to, ...

Dissection and Staining of Drosophila Larval Ovaries

Many organs depend on stem cells for their development during embryogenesis and for maintenance or repair during adult life. Understanding how stem cells form, and how they interact with their environment is therefore crucial for understanding development, homeostasis and disease. The ovary of the fruit fly Drosophila melanogaster has served as an influential model for the interaction of germ line stem cells (GSCs) with their somatic support cells (niche) 1, 2. The known location of the niche and the GSCs, coupled to the ability to genetically manipulate them, has allowed researchers to elucidate a variety of interactions between stem cells and their niches 3-12.
Despite the wealth of information about mechanisms controlling GSC maintenance and differentiation, relatively little is known about how GSCs and their somatic niches form during development. About 18 somatic niches, whose cellular components include terminal filament and cap cells (Figure 1), form during the third larval instar 13-17. GSCs originate from primordial germ cells (PGCs). PGCs proliferate at early larval stages, but following the formation of the niche a subgroup of PGCs becomes GSCs 7, 16, 18, 19. Together, the somatic niche cells and the GSCs make a functional unit that produces eggs throughout the lifetime of the organism.
Many questions regarding the formation of the GSC unit remain unanswered. Processes such as coordination between precursor cells for niches and stem cell precursors, or the generation of asymmetry within PGCs as they become GSCs, can best be studied in the larva. However, a methodical study of larval ovary development is physically challenging. First, larval ovaries are small. Even at late larval stages they are only 100&mu;m across. In addition, the ovaries are transparent and are embedded in a white fat body. Here we describe a step-by-step protocol for isolating ovaries from late third instar (LL3) Drosophila larvae, followed by staining with fluorescent antibodies. We offer some technical solutions to problems such as locating the ovaries, staining and washing tissues that do not sink, and making sure that antibodies penetrate into the tissue. This protocol can be applied to earlier larval stages and to larval testes as well.

Dissection and Staining of Drosophila Larval Ovaries

How niches and stem cells form during development is an important question with practical implications. In the Drosophila ovary, germ line stem cells and their somatic niches form during larval development. This video demonstrates how to dissect, stain and mount female gonads from late third instar (LL3) Drosophila larvae.

Many organs depend on stem cells for their development during embryogenesis and for maintenance or repair during adult life. Understanding how stem cells ...

Isolation of Drosophila melanogaster Testes

The testes of Drosophila melanogaster provide an important model for the study of stem cell maintenance and differentiation, meiosis, and soma-germline interactions. Testes are typically isolated from adult males 0-3 days after eclosion from the pupal case. The testes of wild-type flies are easily distinguished from other tissues because they are yellow, but the testes of white mutant flies, a common genetic background for laboratory experiments are similar in both shape and color to the fly gut. Performing dissection on a glass microscope slide with a black background makes identifying the testes considerably easier. Testes are removed from the flies using dissecting needles. Compared to protocols that use forceps for testes dissection, our method is far quicker, allowing a well-practiced individual to dissect testes from 200-300 wild-type flies per hour, yielding 400-600 testes. Testes from white flies or from mutants that reduce testes size are harder to dissect and typically yield 200-400 testes per hour.

Isolation of Drosophila melanogaster Testes

Drosophila melanogaster testes can be rapidly and efficiently isolated from adult males using dissecting needles. With practice, one can readily isolate in one or two days an amount of testes sufficient for the analysis of DNA or RNA by high throughput sequencing or more traditional molecular biology methods or of protein for antibody- or enzyme-based assays.

The testes of Drosophila melanogaster provide an important model for the study of stem cell maintenance and differentiation, meiosis, and soma-germline ...

Real-Time Imaging of Germline Stem Cells in Drosophila Ex Vivo Germaria Culture

Extended Live Imaging of Female Drosophila melanogaster Germline Stem Cell Niches

Live imaging methods allow the analysis of dynamic cellular processes in detail and in real-time. The Drosophila ovary represents an excellent model to explore the dynamics of a myriad of developmental processes, such as cell division, stemness, differentiation, migration, apoptosis, autophagy, cellular adhesion, etc., over time. Recently, we have implemented an extended ex vivo culture and live imaging of the female Drosophila GSC niche. Using a Drosophila line harboring a GFP::Par-1 transgene as an example, this method allows the visualization of the GSCs&#39; asymmetric division within their niche and the description of the changes in the spectrosome morphology along the cell cycle. Here, we present a detailed protocol for the ex vivo culture of Drosophila germaria, enabling prolonged visualization of the female GSC niche. Importantly, this protocol is broadly applicable to live imaging GSCs with multiple fluorescently tagged proteins of interest that are available in stock centers and/or in the Drosophila research community.

Here, we provide a detailed protocol to perform live imaging of the asymmetric division of germline stem cells (GSCs) in the Drosophila ovarian niche. We use a transgenic line that ubiquitously expresses a green fluorescent protein (GFP) fusion of the spectrosome protein Par-1.

Live imaging methods allow the analysis of dynamic cellular processes in detail and in real-time. The Drosophila ovary represents an excellent model to ...

Ex vivo Culture of Drosophila Pupal Testis and Single Male Germ-line Cysts: Dissection, Imaging, and Pharmacological Treatment

During spermatogenesis in mammals and in Drosophila melanogaster, male germ cells develop in a series of essential developmental processes. This includes differentiation from a stem cell population, mitotic amplification, and meiosis. In addition, post-meiotic germ cells undergo a dramatic morphological reshaping process as well as a global epigenetic reconfiguration of the germ line chromatin&#8212;the histone-to-protamine switch.
Studying the role of a protein in post-meiotic spermatogenesis using mutagenesis or other genetic tools is often impeded by essential embryonic, pre-meiotic, or meiotic functions of the protein under investigation. The post-meiotic phenotype of a mutant of such a protein could be obscured through an earlier developmental block, or the interpretation of the phenotype could be complicated. The model organism Drosophila melanogaster offers a bypass to this problem: intact testes and even cysts of germ cells dissected from early pupae are able to develop ex vivo in culture medium. Making use of such cultures allows microscopic imaging of living germ cells in testes and of germ-line cysts. Importantly, the cultivated testes and germ cells also become accessible to pharmacological inhibitors, thereby permitting manipulation of enzymatic functions during spermatogenesis, including post-meiotic stages.
The protocol presented describes how to dissect and cultivate pupal testes and germ-line cysts. Information on the development of pupal testes and culture conditions are provided alongside microscope imaging data of live testes and germ-line cysts in culture. We also describe a pharmacological assay to study post-meiotic spermatogenesis, exemplified by an assay targeting the histone-to-protamine switch using the histone acetyltransferase inhibitor anacardic acid. In principle, this cultivation method could be adapted to address many other research questions in pre- and post-meiotic spermatogenesis.

Ex vivo Culture of Drosophila Pupal Testis and Single Male Germ-line Cysts: Dissection, Imaging, and Pharmacological Treatment

This protocol describes the dissection and cultivation of intact testes and germ-line cysts from Drosophila melanogaster pupae. This method allows microscopic observation of spermatogenesis ex vivo. Furthermore, we describe a pharmacological assay of the effect of inhibitors on specific stages of germ-cell development in pupal testes.

During spermatogenesis in mammals and in Drosophila melanogaster, male germ cells develop in a series of essential developmental processes. This includes ...

Stimulating and Analyzing Adult Neurogenesis in the Drosophila Central Brain

The molecular and cellular mechanisms underlying neurogenesis in response to disease or injury are not well understood. However, understanding these mechanisms is crucial for developing neural regenerative therapies. Drosophila melanogaster is a leading model for studies of neural development but historically has not been exploited to investigate adult brain regeneration. This is primarily because the adult brain exhibits very low mitotic activity. Nonetheless, penetrating traumatic brain injury (PTBI) to the adult Drosophila central brain triggers the generation of new neurons and new glia. The powerful genetic tools available in Drosophila combined with the simple but rigorous injury protocol described here now make adult Drosophila brain a robust model for neural regeneration research. Provided here are detailed instructions for (1) penetrating injuries to the adult central brain and (2) dissection, immunohistochemistry, and imaging post-injury. These protocols yield highly reproducible results and will facilitate additional studies to dissect mechanisms underlying neural regeneration.

Stimulating and Analyzing Adult Neurogenesis in the Drosophila Central Brain

This article provides detailed protocols for inflicting Penetrating Traumatic Brain Injury (PTBI) to adult Drosophila and examining the resulting neurogenesis.

The molecular and cellular mechanisms underlying neurogenesis in response to disease or injury are not well understood. However, understanding these ...

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

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Methods for Imaging Intracellular pH of the Follicle Stem Cell Lineage in Live Drosophila Ovarian Tissue

Dissection and Staining of Drosophila Pupal Ovaries

Dissection and Live-Imaging of the Late Embryonic Drosophila Gonad

Dissection and Staining of Drosophila Larval Ovaries

Isolation of Drosophila melanogaster Testes

Extended Live Imaging of Female Drosophila melanogaster Germline Stem Cell Niches

Ex vivo Culture of Drosophila Pupal Testis and Single Male Germ-line Cysts: Dissection, Imaging, and Pharmacological Treatment

Stimulating and Analyzing Adult Neurogenesis in the Drosophila Central Brain