Name: thawing, culturing, and cryopreserving drosophila cell lines
Uploaded: 2019-04-16T15:00:00.000+00:00
Duration: 7 min 57 s
Description: Watch this Scientific Journal Video about Thawing, Culturing, and Cryopreserving Drosophila Cell Lines at JoVE.com

We thank the National Institutes of Health (Award NIH P40OD010949) and the research community for utilizing the various D. melanogaster DNA/vector/cell resources curated at the DGRC.

1. Thawing and Reviving Frozen Drosophila Cell Lines
<ol>
	<li>Sterilize the hood by wiping the working surface with 70% ethanol. Dispense 5 mL of the appropriate medium (Table 1) into a 25 cm2 T-flask (T-25).</li>
	<li>Remove the cryovial/ampule from liquid N2 or dry ice. Wipe the cryovial with 70% ethanol, carefully loosen and unseal the ampule.</li>
	<li>Using a Pasteur pipette, withdraw 1 mL of room temperature (RT) media from the T-25 flask. Slowly add the media into the cryovial and gently mix to thaw the frozen cells, ensuring that the cell suspension does not overflow.</li>
	<li>Transfer the entire volume of the thawed cell suspension from the ampule into the T-25 flask. Repeat to ensure the cell suspension has been completely transferred.</li>
	<li>Place the flask in a 25 &#176;C incubator, allowing the cells to settle and adhere for at least 2 h. Examine the cells under a microscope to ensure that most cells have settled on the growing surface. Gently remove old media and replace with 5 mL of fresh media. Return the flask into the incubator.</li>
	<li>On the following day, gently remove the old media and replace with 5 mL of fresh media. Return the culture to the incubator.</li>
</ol>
2. Thawing and Reviving Frozen Drosophila Cell Lines (Alternative)
<ol>
	<li>In a sterile hood, thaw the cells by resuspending the frozen pellet with 1 mL of RT media. Transfer all the thawed cell suspension into a 15 mL conical tube.</li>
	<li>Pellet the cells by centrifugation at 1,000 x g for 5 min. Discard the supernatant and resuspend the cell pellet in 5 mL of fresh media.</li>
	<li>Transfer the entire volume of the cell suspension into a T-25 flask and incubate the culture at 25 &#176;C.</li>
	<li>1 to 2 h later, examine the cells under the microscope to ensure that most cells have settled on the growing surface. On the following day, replace the old media with 5 mL of fresh media and return the culture to the incubator.</li>
</ol>
3. Subculturing Semi-adherent Cells Grown in 100 mm Culture Plates
<ol>
	<li>Sterilize the hood by wiping with 70% ethanol. Bring the sterile materials for subculturing into the hood, including media bottles, pipettes, pipette aid, and culture plates.</li>
	<li>Examine the morphology and confluence of the culture under a microscope. Look for clear signs of microorganismal contaminations in the culture. Determine whether the cells are ready to be passaged, based on the characteristics of the culture: cell density and doubling time, including the last time they were subcultured.</li>
	<li>If the culture appears highly confluent (Figure 1), determine the cell density. In the sterile hood, dislodge the cells from the growing surface by pipetting up to 10 mL of the medium from the plate and dispensing it over the cells. Repeat a few times, ensuring not to create foam, until the growing surface becomes clear. Determine the cell density using a hemocytometer or an automatic particle counter (section 5, Figure 3). Subculture the cells if the cell density is between 5 x 106 and 1 x 107 cells/mL. 
	NOTE: Do not subculture Drosophila cell lines to a cell density below 1 x 106 cells/mL.</li>
	<li>Dilute the cell suspension accordingly using an appropriate medium to a final seeding concentration of at least 1 x 106 cells/mL.
	<ol>
		<li>For routine passaging and maintenance, add an appropriate volume of cell suspension to a pre-determined volume of medium in a new culture plate to achieve the desired seeding cell density.</li>
		<li>For scaling up a culture, transfer all the cell suspension into a large flask. Dilute the cell suspension to the desired cell density with an appropriate volume of the medium. Distribute equal volumes of the diluted cell suspension to new plates. This method minimizes the variations in cell density between plates.</li>
	</ol>
	</li>
	<li>Cover and label the plates with the operator initials, date, split ratio, seeding cell density, cell line identifier, media, passage number and any media additions such as antibiotics.</li>
	<li>Place the plates into a plastic container and return the box to the incubator. 
	NOTE: Table 3 lists the culture vessels commonly used for culturing Drosophila cell lines and the associated working volumes.</li>
</ol>
4. Dislodging Adherent Cells Grown in 100 mm Culture Plates
<ol>
	<li>Transfer all the medium from the plate to a new sterile flask. Save the medium.</li>
	<li>Rinse cells by slowly adding 1 mL&#160;of 0.05% trypsin-EDTA to the plate. Swirl gently to ensure the trypsin solution covers the entire growth surface. Discard the trypsin solution.</li>
	<li>Gently add 1 mL&#160;of 0.05% trypsin-EDTA to the plate. Incubate the plate at 25 &#176;C between 3&#8722;10 min while monitoring for visible signs of the cell layer detaching and sliding off the growing surface.</li>
	<li>Add 9 mL of the saved medium to the plate to stop trypsin activity. Mix the cell suspension to dissociate cell clumps. Once all cells have been dislodged, the growing surface will be clear. 
	NOTE: The use of digestive enzymes such as trypsin aids in passaging strongly adherent cell lines. Trypsin is a mixture of proteases often derived from porcine pancreas and is commercially available in different grades of purity.</li>
</ol>
5. Manual Cell Counting Using the Neubauer Cell Counting Slide
<ol>
	<li>Prepare the hemocytometer slide and coverslip by wiping the surface with 70% alcohol.</li>
	<li>Mix the cell suspension and dispense 15 &#181;L of the cell suspension into the grooved edge of the hemocytometer (Figure 3A) to fill the first chamber of the hemocytometer. Fill the second chamber of the hemocytometer. The cell suspension will be drawn into the counting chamber by capillary action.</li>
	<li>Using a 10x microscope objective, count the cells within the 1 mm2&#160;area in the middle of the grid bound by the parallel lines (Figure 3C,D). To avoid duplicate counting, count the cells that overlay the top and left boundaries, but not cells that cross the right and bottom boundaries of the 200 &#181;m2 squares. Count between 100&#8722;200 cells. Repeat the count with the second chamber.</li>
	<li>Calculate the average of the two counts and determine the cell density according to the following formula: Cell density (cells/mL) = Average cell count (n1 + n2/2) x 104. 
	NOTE: Cell viability is expressed as the percentage of viable cells over total cells. To determine cell viability, mix the cell suspension with an equal volume of trypan blue (0.4%) solution prior to manual or automatic cell counting. Live cells will not take up the dye, while dead cells will be stained blue.</li>
</ol>
6. Cryopreservation of Drosophila Cell Lines
<ol>
	<li>Check the culture for healthy morphology, growth, and the lack of contamination. Harvest the cultures from the mid to late-log growth phase (step 3.3, or section 4). For many Drosophila cell lines, it is approximately between 4 x 106&#160;cells/mL to 8 x 106 cells/mL.</li>
	<li>Transfer the entire cell suspension into a 15 mL or 50 mL conical tube. Collect the cells by centrifugation at 1,000 x g for 5 min and discard the supernatant.</li>
	<li>Resuspend the cell pellet in a volume of freezing medium (Table 4) that will result in a final cell density of at least 4 x 107 cells/mL.</li>
	<li>Add dropwise the appropriate amount of the cryoprotectant dimethyl sulfoxide (DMSO) into the cell suspension such that the final DMSO concentration is 10%. Gently mix the cell suspension.</li>
	<li>Carefully dispense 0.5 mL of the cell suspension into aliquots of the pre-labeled cryovials (~2 x 107 cells/vial). Place the ampules into a freezing container filled with isopropanol (Figure 4A). Transfer the freezing container into a -80 &#176;C freezer overnight to allow the temperature of the cryovials to drop slowly (-1 &#176;C/min) to the freezer temperature.</li>
	<li>Take out the frozen cryovials and rapidly attach them to canes (Figure 4B). Insert the canes containing cryovials into a canister (Figure 4C). Alternatively, place frozen cryovials inside a pre-cooled freezing box (Figure 4D). Store frozen cryovials in the liquid phase of N2 freezers (Figure 4E,F). 
	NOTE: When using freezing media containing DMSO, a delay of up to 30 min at RT is not detrimental to the cells.</li>
</ol>

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The authors have nothing to disclose.

Drosophila cell cultures are primary reagents for high throughput cell-based screens. Their use also complements in vivo genetic research by providing a homogenous population of cells suitable for biochemistry, rapid testing of transgenic constructs prior to injecting into flies, cell biology, microscopy and more recently somatic cell genetic manipulations by genome editing1,2,3,8,9,10.
The viability and recovery of frozen Drosophila cells is sensitive to drastic fluctuations even at low temperatures. The DGRC stores frozen cell lines in the liquid phase of N2 (-196 &#176;C) and transports them in dry ice (-78.5 &#176;C). Frozen ampules that have been transported in dry ice should not be transferred back into liquid N2 or a -80 &#176;C freezer for storage. Instead, the frozen cells should be thawed, reseeded at a high cell density as soon as possible upon arrival (protocol section 1) and cultured for their intended purposes (protocol section 3). If the cell lines are not immediately utilized for experiments, the cell lines should be cryopreserved (protocol section 6) until they are ready for use.
Some cell lines, such as the ML-BG2-c2 and Ras lines need several days to recover from the effects of being revived from the cryopreserved state. A significant amount of cellular debris accompanies these cell lines the first few days after thawing. Left undisturbed, the cells will recover and proliferate. Many Drosophila cell lines at the DGRC have been adapted to grow in M3 based media22. For cell lines that are slow to recover from the effects of thawing, the use of conditioned media may be useful. Conditioned media likely contain growth factors secreted by the cells into the media which may encourage the recovery and proliferation of the cells after thawing.
Cell lines generally follow a stereotypical growth curve consisting of a lag phase, exponential phase, plateau phase and a deterioration phase. Many Drosophila cell lines proliferate in the log-phase of growth when they are cultured at a density between 1 x 106 and 1 x 107 cells/mL at 25 &#176;C. It is essential that cell lines are passaged such that they are always in the exponential growth phase.
The confluence of a culture, expressed as a percentage, describes the growth surface area that is covered by cells. Cell confluence for a cell line depends on its cell shape and size. Distinct cell lines have different morphologies and adherence properties. As a result, different cell lines at approximately similar confluence may have vastly distinct cell density (Figure 1). Culture confluence may not be an ideal indicator for passaging Drosophila cell cultures because Drosophila cell lines continue to proliferate either by piling on top of one another as foci or in suspension even after the growth surface has been covered (Figure 1). However, users experienced with specific cell lines may often use confluence as a rapid visual guide for when to subculture.
While it is possible to grow Drosophila lines at ambient RT between 19&#8722;25 &#176;C, it is not recommended because ambient temperature fluctuations may affect the proliferation rate. The use of a dedicated 25 &#176;C incubator is recommended. The incubator for Drosophila cell cultures does not need to facilitate CO2 gas exchange because Drosophila cell culture media do not use CO2 for buffering. The humidity inside the incubator for culturing cell lines is an important factor not to be overlooked when culturing cells in plates. Depending on the type on incubator and the working environment, it may be necessary to place a beaker of sterile water inside the incubator. To minimize media evaporation, use closed T-flask or store culture plates in a tightly sealed plastic container while inside the incubator.
It is important to develop a schedule for subculturing Drosophila cell lines. To estimate the growth rate and monitor consistency, it is convenient to subculture at an even geometric ratio (split ratio 1:2, 1:4, 1:8). For example, a 10 mL confluent plate of Kc167 cells at 8 x 106 cells/mL can be split at 1:8 ratio to achieve a seeding density of 1 x 106 cells/mL (1.25 mL of cell suspension diluted into 8.75 mL of fresh media). In 72 h, Kc167 cultures are expected to proliferate to a density of 8 x 106 cells/mL, given its doubling time of 24 h. The split ratio therefore is determined to facilitate a convenient subculture routine of up to twice a week, ensuring that the cells are always cultured in their exponential log phase of growth. This allows for a regular schedule for subculturing the cells so that the time to confluence is neither too short nor too long. If the time to confluence is too short, the cells are subcultured at a lower cell density (higher split ratio). Similarly, if the time to reach confluence is too long, the cells are subcultured at a higher cell density (lower split ratio). It is important to note that most Drosophila cell lines are very sensitive to low cell densities (&#60;1 x 105 cells/mL), in which cells hardly proliferate and may eventually die.
Drosophila cell lines vary in growth characteristics and morphology. As a result, cell lines with distinct properties may have to be handled differently. Most Drosophila cell lines are semi-adherent. At lower cell density, they adhere stronger to the growth surface and as the culture becomes confluent, the cells become less adherent and easily detach. This gradual change in cell adherence facilitates easy subculturing of most widely used Drosophila cell lines (Schneider, Kc lines, imaginal disc and CNS lines) as it allows the operator to simply dispense media over the cell monolayer to dislodge them from the growth surface when the culture is dense. For lines that are surface adherent such as the female germ-line stem/ovarian somatic sheath (fGS/OSS) and Ras lines, it is essential to incubate the cells in trypsin for a short duration to aid in detaching the cells from the growth surface.
Media additions for most Drosophila cell lines include fetal calf serum (FCS). Insulin and adult fly extract (FEX) are required for some specific lines. FEX contains undefined components essential to the growth of specific larval imaginal disc lines and the adult ovarian cell lines. The DGRC prepares, and makes available adult FEX derived from 1 week old Oregon-R-modENCODE flies (RRID: BDSC_25211) in 2.5 mL and 10 mL aliquots. The DGRC also provides instructions for small scale FEX preparation on its website &#60;https://dgrc.bio.indiana.edu/include/file/additions_to_medium.pdf&#62;. FEX preparation, however, is time-consuming and requires a large quantity of adult flies.
The cryopreservation of Drosophila cell lines saves time and reagents for the maintenance of cell lines not in immediate use. Cryopreservation is achieved by slowly freezing the cells (-1 &#176;C/min) to -80 &#176;C in a medium containing DMSO, a cryoprotective agent. The slow cooling step is critical for successful cryopreservation. In a -80 &#176;C freezer, the ampule of cells is cooled at a rate of -1 &#176;C/min when placed in a freezing container filled with isopropanol. Starting at 25 &#176;C ambient temperature, it will take up to 2 h for the temperature in the ampules to reach -80 &#176;C. It is recommended to leave the ampules to freeze overnight.
Frozen ampules must then be rapidly transferred into the liquid phase of nitrogen for prolonged storage. At ambient temperature, the cryovial will reheat rapidly at approximately 10 &#176;C/min and the viability will be compromised at above -50 &#176;C23. To keep the transfer rapid, handle ampules in small batches to minimize the exposure to ambient temperature. Alternatively, place the frozen cryovials on dry ice while preparing for their transfer into liquid N2. If liquid nitrogen is not available, the cells may be stored in a -80 &#176;C freezer, although with a risk of significant deterioration over time.
Cell density is critical for successful cryopreservation and the subsequent revival of cell lines. In general, new cell lines should be frozen to create the initial freeze (1&#8722;3 ampules) as soon as an excess of cells becomes available. Once the cell line has been further cultured stably, a frozen stock of 10&#8722;20 ampules should be created. This stock is then thawed to check for its post-freeze cell recovery and viability, after which it is propagated for experimentations or to replace the stock when the number of frozen stock ampules falls below five. Finally, it is important to validate that the thawed cells retain the characteristics of its parental stock as cell lines are known to evolve3,24.
In conclusion, this article presents a primer for working with Drosophila cell cultures by providing the fundamental information on the various lines, best practices, and audiovisual protocols for the basic handling of Drosophila cell lines. This accessible resource is meant to smoothly ease the introduction to working with cultured Drosophila cells and to complement existing training guides at any research laboratory.

The use of Drosophila cultured cells complements in vivo fly genetic analysis and serves as a primary inquiry tool for addressing many basic biological questions1,2,3. Drosophila cell lines offer unique homogenous populations of cells derived from different tissue sources with distinct genetic backgrounds. Cell lines are suitable for many applications including transgenic gene expression, genomics, transcriptomics, proteomics, metabolomics, high throughput RNA interference (RNAi) screens, cell biology and microscopy. Importantly, the use of Drosophila cell culture facilitates the characterization of the immediate temporal responses to known stimuli. Furthermore, Drosophila cell culture is amenable to CRISPR-Cas9 genome editing, making it relatively easy to create new cell lines with specific genome modifications4,5,6,7.
The Drosophila Genomics Resource Center (DGRC) serves as a repository and distribution center for Drosophila cell lines. One of the goals of the DGRC is to assist members of the research community in using Drosophila cell culture resources. This article presents basic protocols for the handling of Drosophila cell lines. It complements existing resources to help researchers become comfortable with handling Drosophila cell cultures and achieve a level of independence in their experiments1,2,8,9,10.
The most commonly used Drosophila cell lines are: Schneider lines11, Kc16712, Mitsubishi/Miyake imaginal disc and central nervous system (CNS) lines13,14, Milner laboratory imaginal disc lines15, the adult ovarian cell lines16,17, and the Ras lines18 (Table 1). The Schneider and Kc167 lines are general all-purpose cell lines for use in biochemistry, recombinant transgenic gene expression, and reverse genetic screens. The Mitsubishi/Miyake laboratory (ML) lines were derived from either the larval imaginal discs or central nervous system (CNS) and they have been useful for studies related to neurosecretion, transcription regulation, and RNA processing. The Milner (CME) disc lines have been important for studying signal transduction. The fGS/OSS cell lines derived from mutant adult ovaries remain important reagents to study the impact of non-coding small RNA biology in germ cell maintenance and differentiation17,19. Lastly, the Ras lines are unique because these are cell lines derived from embryos ectopically expressing the Ras oncogene. They have the transcriptional signature of muscle precursor cells and expresses active piRNA machinery20. Recent review articles and book chapters cover the applications of these popular cell lines with more details2,3,9.
All these cell lines can be subcultured and frozen. There are slight but important different requirements for how each cell line is maintained and prepared for cryopreservation. For example, distinct cell lines require different media and supplements (Table 1). The lines also vary in surface adherence properties, morphologies (Figure 1 and Figure 2), genotype and doubling time (Table 2). We present basic protocols and highlight the unique differences for handling the various widely used Drosophila cell lines.

<table><tbody><tr><td>100 mm tissue culture plates</td><td>Corning&amp;nbsp;</td><td>430167</td><td>Subculturing</td></tr><tr><td>25 cm&lt;sup&gt;2&lt;/sup&gt; T-flask</td><td>Corning&amp;nbsp;</td><td>430168</td><td>Subculturing</td></tr><tr><td>35HC Liquid Nitrogen Storage Tank</td><td>Taylor-Wharton</td><td>35HCB-11M</td><td>Cryopreservation</td></tr><tr><td>Automated Cell counter</td><td>BIO-RAD</td><td>TC20</td><td>Counting</td></tr><tr><td>Bactopeptone</td><td>BD BioSciences</td><td>211677</td><td>Medium additions</td></tr><tr><td>Counting Slides</td><td>BIO-RAD</td><td>145-0011</td><td>Counting</td></tr><tr><td>Cryovial 1 mL</td><td>Greiner&amp;nbsp;</td><td>123263</td><td>Cryopreservation</td></tr><tr><td>DMSO</td><td>Sigma Aldrich</td><td>D5879</td><td>Cryopreservation</td></tr><tr><td>Freezing Box</td><td>Nalgene</td><td>5029-0909</td><td>Cryopreservation</td></tr><tr><td>Freezing Container</td><td>Fisher Scientific</td><td>15-350-50</td><td>Cryopreservation</td></tr><tr><td>Hematocytometer</td><td>Fisher Scientific</td><td>#0267110</td><td>Counting</td></tr><tr><td>Human Insulin</td><td>Millipore Sigma</td><td>I9278</td><td>Medium additions</td></tr><tr><td>Hyclone CCM3 media</td><td>GE Healthcare Life Sciences</td><td>SH30061.03</td><td>Medium</td></tr><tr><td>Hyclone Fetal Bovine Serum</td><td>GE Healthcare Life Sciences</td><td>SH30070.03</td><td>Medium additions</td></tr><tr><td>L-Glutamic acid potassium salt monohydrate</td><td>Millipore Sigma</td><td>G1149</td><td>Medium additions</td></tr><tr><td>L-Glutathione reduced</td><td>Millipore Sigma</td><td>G6013</td><td>Medium additions</td></tr><tr><td>Potassium Bicarbonate</td><td>Millipore Sigma</td><td>237205</td><td>Medium additions</td></tr><tr><td>Select Yeast Extract&amp;nbsp;</td><td>Millipore Sigma</td><td>Y1000</td><td>Medium additions</td></tr><tr><td>Shields and Sang&#039;s M3 Insect medium</td><td>Millipore Sigma</td><td>S8398</td><td>Medium</td></tr><tr><td>Trpsin-EDTA (0.05 %), phenol red&amp;nbsp;</td><td>ThermoFisher Scientific</td><td>25300054</td><td>Subculturing</td></tr><tr><td>Trypan Blue (0.4%)</td><td>BIO-RAD</td><td>145-0013</td><td>Counting</td></tr></tbody></table>

thawing, culturing, and cryopreserving drosophila cell lines

There are currently over 160 distinct Drosophila cell lines distributed by the Drosophila Genomics Resource Center (DGRC). With genome engineering, the number of novel cell lines is expected to increase. The DGRC aims to familiarize researchers with using Drosophila cell lines as an experimental tool to complement and drive their research agenda. Procedures for working with a variety of Drosophila cell lines with distinct characteristics are provided, including protocols for thawing, culturing, and cryopreserving cell lines. Importantly, this publication demonstrates the best practices required to work with Drosophila cell lines to minimize the risk of contaminations from adventitious microorganisms or from other cell lines. Researchers who become familiar with these procedures will be able to delve into the many applications that use Drosophila cultured cells including biochemistry, cell biology and functional genomics.

It is important to thaw frozen Drosophila cells rapidly and culture them at a cell density that brings the culture back into the growth phase. If the procedures for cryopreservation and thawing are adhered to, the cell density in the T-25 flask will at least equal 4 x 106 cells/mL. One to two hours after thawing, most Drosophila cell lines will begin to attach to the growing surface. Under the circumstance in which most of the cells have not attached on the growing surface within two hours after thawing, it is recommended to incubate the cells overnight before changing the media.
The goal of subculturing is to maintain cells in the healthy exponential log-phase of the growth curve. The criteria for subculturing depend on the visible lack of microorganismal contamination, cell density, and the need to establish a regular maintenance schedule. It is important to first assess the health of the cells and determine the absence of adventitious contaminants prior to freezing. Most bacterial and fungal contaminants are easy to detect simply by visual inspections. Contaminated cultures can be identified by an increase in media turbidity. Under the microscope, contaminants may appear as bacterial rods, cocci, budding yeast cells or string-like fungal hyphae. Other sources of contamination such as the non-cytopathic mycoplasma cannot be visually detected and can be routinely tested by PCR-based assays21.
The confluence of a cell line can be determined visually (Figure 1). Fast growing cell lines reach confluence early and need to be passaged regularly. Such lines are subcultured up to twice a week. In contrast, slow growing cells are passaged at least once every two weeks or longer. However, the cells need to be fed fresh media every week. This is to prevent media exhaustion and to dilute metabolic waste products from the cells. Cell lines derived from varying tissue sources differ in their morphology (Figure 2), adherence properties, media requirements (Table 1) and doubling time (Table 2). Table 5, Table 6, Table 7, and Table 8 list the recipes for the various Drosophila cell culture media.
Cell counting ensures an accurate seeding density and a predictable routine for subculturing. For quantitative experiments, cell counting is essential. Cells are counted either by using a hemocytometer (Figure 3A) or an automated particle counter (Figure 3B). If using an automated counter, follow the manufacturer&#39;s instructions. Counting cells manually using a hemocytometer is economical and easy. The number of cells enclosed in the middle Neubauer grids are counted and the cell density is calculated; For example, n = 214 cells, resulting in a cell density of 2.14 x 106 cells/mL (Figure 3D).
Cell suspension from two 100 mm plates, each containing 10 mL of cell suspension at 4 x 106 cells/mL are collected and resuspended in 2 mL of freezing media to achieve a density of 4 x 107 cells/mL. Each frozen cryovial with 0.5 mL of cell suspension contains 2 x 107 cells. This will result in a culture with 4 x 106 cells/mL when thawed according to the protocol section 1.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/59459/59459fig1.jpg" /> 
Figure 1:&#160;Representative images of three distinct Drosophila cell lines at different confluence and cell densities. (A) S2-DGRC culture at 1 x 106 cells/mL. (A&#39;) S2-DGRC culture at 4.5 x 106 cells/mL. (B) ML-BG2-c2 culture at 2 x 106 cells/mL. (B&#39;) ML-BG2-c2 culture at 8 x 106 cells/mL in which cells are piling and aggregating as foci. (C) OSS culture at 1 x 106 cells/mL. (C&#39;) OSS culture at 4 x 106 cells/mL. Cells in suspension are not captured on the same focal plane. Scale bar = 100 &#181;m. <a href="https://www.jove.com/files/ftp_upload/59459/59459fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/59459/59459fig2.jpg" /> 
Figure 2: Representative images of the eight distinct Drosophila cell lines. (A) Round embryo-derived S2-DGRC. (B) Round embryo-derived Kc167. (C) Round larval CNS-derived ML-BG2-c2. (D) Round larval spindle-shaped ML-BG3-c2. (E) CME L1, a cell line derived from the larval leg imaginal discs, is smaller and has round/fusiform morphology. (F) OSS, a cell line derived from adult ovaries, displays spindle-shaped morphology. (G) Spindle-shaped RasV12 cell line expressing activated Ras. (H) RasV12; wtsRNAi (WRR1), a cell line expressing activated Ras and double-stranded RNA targeting the tumor suppressor warts (wts), displays epithelial characteristics. Scale bar = 50 &#181;m. <a href="https://www.jove.com/files/ftp_upload/59459/59459fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/59459/59459fig3.jpg" /> 
Figure 3: Cell density can be counted manually using a hemocytometer or automatically using an automated particle counter. (A) A hemocytometer with two chambers. (B) An automated cell counter displaying the output of a cell count. (C) The improved Neubauer cell counting grid viewed under a 10x objective. Count cells bound by the 0.1 mm3 central grid (red dashed-line square). (D) The central grid on the hemocytometer filled with cells for counting. Scale bar = 1 mm (C);&#160;0.2 mm (D). <a href="https://www.jove.com/files/ftp_upload/59459/59459fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/59459/59459fig4.jpg" /> 
Figure 4: Equipment for cryopreservation. (A) A freezing container stores the ampules in an upright position for slow freezing. (B) A metal cane for holding frozen ampules. (C) A canister for holding canes. (D) A plastic freezing box (cryobox). (E) A canister holding multiple canes inserted into a liquid N2 storage tank. (F) A liquid N2 storage tank. <a href="https://www.jove.com/files/ftp_upload/59459/59459fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Cell Strain</td>
			<td>Media</td>
			<td>Adherence</td>
			<td>Trypsin</td>
		</tr>
		<tr>
			<td>Schneider Lines</td>
			<td rowspan="2">M3 + BPYE + 10% fetal calf serum (FCS), pH 6.6</td>
			<td rowspan="3">Semi-adherent</td>
			<td rowspan="3">No</td>
		</tr>
		<tr>
			<td>(S2R+, S2-DRSC, S2-DGRC, Sg4)11</td>
		</tr>
		<tr>
			<td></td>
			<td>Schneider&#8217;s media+ + 10% FCS</td>
		</tr>
		<tr>
			<td rowspan="2">Kc lines (Kc167, Kc7E10)21,22</td>
			<td>M3 + BPYE + 5% FCS, pH 6.6</td>
			<td rowspan="2">Semi-adherent</td>
			<td rowspan="2">No</td>
		</tr>
		<tr>
			<td>Hyclone-CCM3, pH 6.2</td>
		</tr>
		<tr>
			<td rowspan="3">Imaginal disc and CNS lines (ML-lines)13,14</td>
			<td>M3 + BPYE + 10% FCS, pH 6.6</td>
			<td rowspan="3">Semi-adherent</td>
			<td rowspan="3">No</td>
		</tr>
		<tr>
			<td>10 &#181;g/mL insulin</td>
		</tr>
		<tr>
			<td></td>
		</tr>
		<tr>
			<td rowspan="4">Milner imaginal disc lines (CME-lines)15</td>
			<td>M3 + 2% FCS&#160;</td>
			<td rowspan="4">Semi-adherent</td>
			<td rowspan="4">No</td>
		</tr>
		<tr>
			<td>5 &#181;g/mL insulin&#160;</td>
		</tr>
		<tr>
			<td>2.5% fly extract</td>
		</tr>
		<tr>
			<td></td>
		</tr>
		<tr>
			<td rowspan="6">fGS/OSS16</td>
			<td>M3 + 10% FCS, pH 6.8</td>
			<td rowspan="6">Adherent</td>
			<td rowspan="6">*</td>
		</tr>
		<tr>
			<td>10 &#181;g/mL insulin</td>
		</tr>
		<tr>
			<td>1 mg/mL C5H8KNO4&#160;&#160;</td>
		</tr>
		<tr>
			<td>0.5 mg/mL KHCO3&#160;</td>
		</tr>
		<tr>
			<td>0.6 mg/mL glutathione&#160;</td>
		</tr>
		<tr>
			<td>10% fly extract</td>
		</tr>
		<tr>
			<td>RasV12 lines18</td>
			<td>M3 + BPYE + 10% FCS, pH 6.6</td>
			<td>Adherent</td>
			<td>Yes</td>
		</tr>
	</tbody>
</table>
Table 1:&#160;The properties and media requirements of various Drosophila cell lines. Different isolates of semi-adherent Schneider lines including S2R+, S2-Drosophila RNAi Screening Center (DRSC), S2-Drosophila Genomics Resource Center (DGRC), and Sg4 are commonly used cell lines that proliferate robustly when cultured in M3 media + Bactopetone yeast extract (BPYE) supplemented with 10% fetal calf serum (FCS). Alternatively, Schneider&#39;s media (pH 6.7-6.8) is often used in place of M3+BPYE. The Kc lines proliferate in either M3 + BPYE (5% FCS) or serum-free CCM3 media. The ML imaginal disc and central nervous system (CNS) lines require insulin supplementation for proliferation. The Milner imaginal disc lines require both insulin and fly extract supplementation. Adherent fGS/OSS cell lines require insulin, a higher concentration of fly extract as well as glutathione for growth. Adherent RasV12 lines grow well in M3 + BPYE (10% FCS). Trypsin is used to dislodge adherent cell lines from the growth surface.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Cell line (Stock #)</td>
			<td>Genotype</td>
			<td>Doubling time (h)*</td>
			<td>Tissue Source</td>
		</tr>
		<tr>
			<td>S2R+ (150)</td>
			<td>OreR</td>
			<td>39</td>
			<td>Late embryos</td>
		</tr>
		<tr>
			<td>S2-DGRC (6)</td>
			<td>OreR</td>
			<td>23</td>
			<td>Late embryos</td>
		</tr>
		<tr>
			<td>S2-DRSC (181)</td>
			<td>OreR</td>
			<td>46</td>
			<td>Late embryos</td>
		</tr>
		<tr>
			<td>Kc167 (1)</td>
			<td>e/se</td>
			<td>22</td>
			<td>6&#8722;12 h embryos</td>
		</tr>
		<tr>
			<td>ML-BG2-c2 (53)</td>
			<td>y v f mal</td>
			<td>48</td>
			<td>3rd instar larval CNS</td>
		</tr>
		<tr>
			<td>ML-BG3-c2 (68)</td>
			<td>y v f mal</td>
			<td>104</td>
			<td>3rd instar larval CNS</td>
		</tr>
		<tr>
			<td>ML-DmD8 (92)</td>
			<td>y v f mal</td>
			<td>66</td>
			<td>3rd instar larval wing disc</td>
		</tr>
		<tr>
			<td>CME W1 Cl.8+ (151)</td>
			<td>OreR</td>
			<td>46</td>
			<td>3rd instar larval wing disc</td>
		</tr>
		<tr>
			<td>CME L1 (156)</td>
			<td>OreR</td>
			<td>47</td>
			<td>3rd instar larval leg disc</td>
		</tr>
		<tr>
			<td>OSS (190)</td>
			<td>bamD86</td>
			<td>45</td>
			<td>Adult bam mutant ovaries</td>
		</tr>
		<tr>
			<td>RasV12 lines</td>
			<td>UAS-GFP; P(UAS-Ras85D.V12)/ P(Act5C-GAL4)17bFO1</td>
			<td>41&#8722;65</td>
			<td>Embryo</td>
		</tr>
	</tbody>
</table>
Table 2:&#160;Genotype, doubling time, and tissue sources of widely used Drosophila cell lines. The tissue genotype, source and population doubling time of commonly used cell lines are presented. Doubling time is based on growth in the recommended media at 25 &#176;C.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Culture vessel</td>
			<td>Volume of media (mL)</td>
		</tr>
		<tr>
			<td>12.5 cm2 T-flask</td>
			<td>2.5</td>
		</tr>
		<tr>
			<td>25 cm2 T-flask</td>
			<td>5</td>
		</tr>
		<tr>
			<td>75 cm2 T-flask</td>
			<td>15</td>
		</tr>
		<tr>
			<td>35 mm plate</td>
			<td>1</td>
		</tr>
		<tr>
			<td>60 mm plate</td>
			<td>4</td>
		</tr>
		<tr>
			<td>100 mm plate</td>
			<td>10</td>
		</tr>
		<tr>
			<td>384-well plate*</td>
			<td>0.04/well</td>
		</tr>
		<tr>
			<td>96-well plate*</td>
			<td>0.1/well</td>
		</tr>
		<tr>
			<td>48-well plate*</td>
			<td>0.3/well</td>
		</tr>
		<tr>
			<td>24-well plate*</td>
			<td>0.5/well</td>
		</tr>
		<tr>
			<td>12-well plate</td>
			<td>1.0/well</td>
		</tr>
		<tr>
			<td>6-well plate</td>
			<td>2.0/well</td>
		</tr>
	</tbody>
</table>
Table 3: Culture vessels and the recommended media volumes. Culture vessels of various sizes are available for culturing Drosophila cells. The appropriate media volumes (mL) are recommended for each vessel. Seal multi-well plates containing less than 0.5 mL of cell suspension with paraffin film to reduce media loss due to evaporation.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td></td>
			<td>Volume</td>
		</tr>
		<tr>
			<td>M3 + BPYE, pH 6.6</td>
			<td>70 mL</td>
		</tr>
		<tr>
			<td>Heat inactivated FCS</td>
			<td>20 mL</td>
		</tr>
		<tr>
			<td>Sterile filtered DMSO*</td>
			<td>10 mL</td>
		</tr>
	</tbody>
</table>
Table 4: Recipe for preparing 100 mL of freezing medium (M3 + BPYE, 20% FCS, 10% DMSO). Prepare freezing media as needed and avoid storing freezing media containing DMSO for prolonged period.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>M3 + BPYE medium</td>
			<td>Amount</td>
		</tr>
		<tr>
			<td>Shields and Sang&#8217;s M323</td>
			<td>1 bottle</td>
		</tr>
		<tr>
			<td>KHCO3</td>
			<td>0.5 g</td>
		</tr>
		<tr>
			<td>Select yeast extract&#160;</td>
			<td>1.0 g</td>
		</tr>
		<tr>
			<td>Bactopeptone</td>
			<td>2.5 g</td>
		</tr>
		<tr>
			<td>Sterile purified water&#160;</td>
			<td>1000 mL</td>
		</tr>
	</tbody>
</table>
Table 5:&#160;Recipe for preparing 1 L of M3 + BPYE tissue culture medium. Adjust pH to 6.6. Sterilize by passing the medium through a 0.22 &#181;m filter.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Base M3 medium for fGS/OSS cell line</td>
			<td>Amount</td>
		</tr>
		<tr>
			<td>Shields and Sang M3</td>
			<td>1 bottle</td>
		</tr>
		<tr>
			<td>KHCO3</td>
			<td>0.5 g</td>
		</tr>
		<tr>
			<td>C5H8KNO4&#160;&#160;</td>
			<td>1.0 g</td>
		</tr>
		<tr>
			<td>Sterile purified water&#160;</td>
			<td>1,000 mL</td>
		</tr>
	</tbody>
</table>
Table 6:&#160;Recipe for 1 L of fGS/OSS M3 base medium. Adjust pH to 6.8. Sterilize by passing the medium through a 0.22 &#181;m filter.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Hyclone-CCM3</td>
			<td>Amount</td>
		</tr>
		<tr>
			<td>CCM3 powder</td>
			<td>28.6 g</td>
		</tr>
		<tr>
			<td>NaHCO3</td>
			<td>0.35 g</td>
		</tr>
		<tr>
			<td>10 N NaOH</td>
			<td>2.5 mL</td>
		</tr>
		<tr>
			<td>CaCl2</td>
			<td>0.5 g</td>
		</tr>
		<tr>
			<td>Sterile purified water&#160;</td>
			<td>1,000 mL</td>
		</tr>
	</tbody>
</table>
Table 7:&#160;Recipe for 1 L of Hyclone-CCM3 tissue culture medium. Adjust pH to 6.2. Sterilize by passing the medium through a 0.22 &#181;m filter.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td></td>
			<td>M3 + BPYE + 10% FCS</td>
			<td>Miyake disc and CNS lines medium</td>
			<td>Milner disc lines medium</td>
			<td>fGS/OSS complete medium</td>
		</tr>
		<tr>
			<td>M3 + BPYE, pH 6.6</td>
			<td>90 mL</td>
			<td>90 mL</td>
			<td>-</td>
			<td>-</td>
		</tr>
		<tr>
			<td>Heat inactivated FCS*</td>
			<td>10 mL</td>
			<td>10 mL</td>
			<td>2 mL</td>
			<td>10 mL</td>
		</tr>
		<tr>
			<td>Insulin (10 mg/mL)</td>
			<td>-</td>
			<td>100 &#181;L</td>
			<td>50 &#181;L</td>
			<td>100 &#181;L</td>
		</tr>
		<tr>
			<td>Fly extract</td>
			<td>-</td>
			<td>-</td>
			<td>2.5 mL</td>
			<td>10 mL</td>
		</tr>
		<tr>
			<td>Glutathione (60 mg/mL)</td>
			<td>-</td>
			<td>-</td>
			<td></td>
			<td>1 mL</td>
		</tr>
		<tr>
			<td>M3, pH 6.6&#160;</td>
			<td>-</td>
			<td>-</td>
			<td>97.5 mL</td>
			<td>-</td>
		</tr>
		<tr>
			<td>fGS/OSS M3, pH 6.8</td>
			<td>-</td>
			<td>-</td>
			<td></td>
			<td>79 mL</td>
		</tr>
	</tbody>
</table>
Table 8:&#160;Recipe for preparing 100 mL of various common Drosophila cell culture media. Incubate FCS at 56 &#176;C for 1 h&#160;and shake every five minutes to heat-inactivate complement proteins.

Watch this Scientific Journal Video about Thawing, Culturing, and Cryopreserving Drosophila Cell Lines at JoVE.com

Thawing, Culturing, and Cryopreserving Drosophila Cell Lines

Drosophila cell lines are important reagents for both fundamental and biomedical research. This article provides protocols for thawing, subculturing, and the cryopreservation of commonly used Drosophila cell lines to assist researchers in incorporating the use of these reagents in their research.

Thawing, Culturing, and Cryopreserving Drosophila Cell Lines

There are currently over 160 distinct Drosophila cell lines distributed by the Drosophila Genomics Resource Center (DGRC). With genome engineering, the ...

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Research

JoVE Journal

Developmental Biology

80.6K Views.  Indiana University Bloomington. Drosophila cell lines are important reagents for both fundamental and biomedical research. This article provides protocols for thawing, subculturing, and the cryopreservation of commonly used Drosophila cell lines to assist researchers in incorporating the use of these reagents in their research.

Video: Thawing, Culturing, and Cryopreserving Drosophila Cell Lines

Primary Neuronal Cultures from the Brains of Late Stage Drosophila Pupae

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

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

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

Biology

Preparation of Neuronal Cultures from Midgastrula Stage Drosophila Embryos

This video illustrates the procedure for making primary neuronal cultures from midgastrula stage Drosophila embryos. The methods for collecting embryos and their dechorionation using bleach are demonstrated. Using a glass pipet attached to a mouth suction tube, we illustrate the removal of all cells from single embryos. The method for dispersing cells from each embyro into a small (5 l) drop of medium on an uncoated glass coverslip is demonstrated. A view through the microscope at 1 hour after plating illustrates the preferred cell density. Most of the cells that survive when grown in defined medium are neuroblasts that divide one or more times in culture before extending neuritic processes by 12-24 hours. A view through the microscope illustrates the level of neurite outgrowth and branching expected in a healthy culture at 2 days in vitro. The cultures are grown in a simple bicarbonate based defined medium, in a 5% CO2 incubator at 22-24&deg;C. Neuritic processes continue to elaborate over the first week in culture and when they make contact with neurites from neighboring cells they often form functional synaptic connections. Neurons in these cultures express voltage-gated sodium, calcium, and potassium channels and are electrically excitable. This culture system is useful for studying molecular genetic and environmental factors that regulate neuronal differentiation, excitability, and synapse formation/function.

This video demonstrates the preparation of primary neuronal cultures from midgastrula stage Drosophila embryos. Views of live cultures show cells 1 hour after plating and differentiated neurons after 2 days of growth in a bicarbonate-based defined medium. The neurons are electrically excitable and form synaptic connections.

This video illustrates the procedure for making primary neuronal cultures from midgastrula stage Drosophila embryos. The methods for collecting embryos ...

Freezing, Thawing, and Packaging Cells for Transport

Cultured mammalian cells are used extensively in cell biology studies. It requires a number of special skills in order to be able to preserve the structure, function, behavior, and biology of the cells in culture. This video describes the basic skills required to freeze and store cells and how to recover frozen stocks. 

Cultured mammalian cells are used extensively in cell biology studies. This video describes the basic skills required to freeze and store cells and how to recover frozen stocks.

Cultured mammalian cells are used extensively in cell biology studies. It requires a number of special skills in order to be able to preserve the ...

Medium-scale Preparation of Drosophila Embryo Extracts for Proteomic Experiments

Analysis of protein-protein interactions (PPIs) has become an indispensable approach to study biological processes and mechanisms, such as cell signaling, organism development, and disease. It is often desirable to obtain PPI information using in vivo material, to gain the most natural and unbiased view of the interaction networks. The fruit fly Drosophila melanogaster is an excellent platform to study PPIs in vivo, and lends itself to straightforward approaches to isolating material for biochemical experiments. In particular, fruit fly embryos represent a convenient type of tissue to study PPIs, due to the ease of collecting animals at this developmental stage and the fact that the majority of proteins are expressed in embryogenesis, thus providing a relevant environment to reveal most PPIs. Here we present a protocol for collection of Drosophila embryos at medium scale (0.5-1 g), which is an ideal amount for a wide range of proteomic applications, including analysis of PPIs by affinity purification-mass spectrometry (AP-MS). We describe our designs for 1 L and 5 L cages for embryo collections that can be easily and inexpensively set up in any laboratory. We also provide a general protocol for embryo collection and protein extraction to generate lysates that can be directly used in downstream applications such as AP-MS. Our goal is to provide an accessible means for all researchers to carry out the analyses of PPIs in vivo.

Medium-scale Preparation of Drosophila Embryo Extracts for Proteomic Experiments

The goal of this protocol is to provide a straightforward and inexpensive approach to collecting Drosophila embryos at medium scale (0.5-1 g) and preparing protein extracts that can be used in downstream proteomic applications, such as affinity purification-mass spectrometry (AP-MS).

Analysis of protein-protein interactions (PPIs) has become an indispensable approach to study biological processes and mechanisms, such as cell signaling, ...

Cryopreservation of PGCs for Long-Term Preservation of Drosophila Strains

Primordial Germ Cell Cryopreservation and Revival of Drosophila Strains

Drosophila strains must be maintained by the frequent transfer of adult flies to new vials. This carries a danger of mutational deterioration and phenotypic changes. Development of an alternative method for long-term preservation without such changes is therefore imperative. Despite previous successful attempts, cryopreservation of Drosophila embryos is still not of practical use because of low reproducibility. Here, we describe a protocol for primordial germ cell (PGC) cryopreservation and strain revival via transplantation of cryopreserved PGCs into agametic Drosophila melanogaster (D. melanogaster) host embryos. PGCs are highly permeable to cryoprotective agents (CPAs), and developmental and morphological variation among strains is less problematic than in embryo cryopreservation. In this method, PGCs are collected from approximately 30 donor embryos, loaded into a needle after CPA treatment, and then cryopreserved in liquid nitrogen. To produce donor-derived gametes, the cryopreserved PGCs in a needle are thawed and then deposited into approximately 15&#160;agametic host embryos. A frequency of at least 15% fertile flies was achieved with this protocol, and the number of progeny per fertile couple was always more than enough to revive the original strain (the average progeny number being 77.2 &#177; 7.1), indicating the ability of cryopreserved PGCs to become germline stem cells. The average number of fertile flies per needle was 1.1 &#177; 0.2, and 9 out of 26 needles produced two or more fertile progeny. It was found that 11 needles are enough to produce 6 or more progeny, in which at least one female and one male are likely included. The agametic host makes it possible to revive the strain quickly by simply crossing newly emerged female and male flies. In addition, PGCs have the potential to be used in genetic engineering applications, such as genome editing.

Author Spotlight: PGC Cryopreservation &#8211; An Alternative Approach Towards Long-Term Preservation of Drosophila Strains 

A long-term preservation method for Drosophila strains as an alternative to the frequent transfer of adult flies to fresh food vials is highly desirable. This protocol describes the cryopreservation of Drosophila primordial germ cells and strain revival via their transplantation to agametic host embryos.

Drosophila strains must be maintained by the frequent transfer of adult flies to new vials. This carries a danger of mutational deterioration and ...

Genetics

A Cell-based Assay to Investigate Non-muscle Myosin II Contractility via the Folded-gastrulation Signaling Pathway in Drosophila S2R+ Cells

We have developed a cell-based assay using Drosophila cells that recapitulates apical constriction initiated by folded gastrulation (Fog), a secreted epithelial morphogen. In this assay, Fog is used as an agonist to activate Rho through a signaling cascade that includes a G-protein-coupled receptor (Mist), a G&#945;12/13 protein (Concertina/Cta), and a PDZ-domain-containing guanine nucleotide exchange factor (RhoGEF2). Fog signaling results in the rapid and dramatic reorganization of the actin cytoskeleton to form a contractile purse string. Soluble Fog is collected from a stable cell line and applied ectopically to S2R+ cells, leading to morphological changes like apical constriction, a process observed during developmental processes such as gastrulation. This assay is amenable to high-throughput screening and, using RNAi, can facilitate the identification of additional genes involved in this pathway.

A Cell-based Assay to Investigate Non-muscle Myosin II Contractility via the Folded-gastrulation Signaling Pathway in Drosophila S2R+ Cells

Here we describe a contractility assay using Drosophila S2R+ cells. The application of an exogenous ligand, folded gastrulation (Fog), leads to the activation of the Fog signaling pathway and cellular contractility. This assay can be used to investigate the regulation of cellular contractility proteins in the Fog signaling pathway.

We have developed a cell-based assay using Drosophila cells that recapitulates apical constriction initiated by folded gastrulation (Fog), a secreted ...

Novel And Efficient Method for Drosophila Heart Fluorescence Staining with Cryosectioning

Drosophila heart models are widely employed in studying cardiac aging and modeling&#160;human cardiac diseases. However, the dissection of Drosophila hearts before imaging is a meticulous time-intensive process that requires advanced training and motor skills. To address these challenges, we present an innovative protocol that utilizes cryosectioning for the fluorescence imaging of Drosophila heart tissue. The protocol has been demonstrated in imaging the adult Drosophila heart but could be adapted for developmental stages. The method enhances both the efficiency and accessibility of fluorescence staining while preserving the integrity of the tissue. This protocol simplifies the process without compromising the quality of imaging, thereby reducing the dependency on technicians with highly developed training and motor skills. Specifically, we replace complex techniques, such as capillary vacuum suction, with more straightforward methods like tissue embedding. This approach allows for the visualization of cardiac structures with greater ease and reproducibility. We demonstrate the utility of this protocol by effectively detecting key cardiac markers and&#160;achieving high-resolution fluorescence and immunostaining imaging that unveils intricate details of heart morphology and cellular organization. This method provides a robust and accessible tool for researchers exploring Drosophila cardiac biology, facilitating detailed analyses of heart development, function, and disease models.

The Drosophila heart sectioning and fluorescence imaging protocol simplifies studying heart structure and pathologies. This approach involves straightforward sectioning, staining, and imaging, bypassing the technical expertise needed for traditional dissection. It enhances accessibility, making Drosophila a more widely usable model for cardiac-related research within the broader scientific community.

Drosophila heart models are widely employed in studying cardiac aging and modeling&#160;human cardiac diseases. However, the dissection of Drosophila ...

Primary Cell Cultures from Drosophila Gastrula Embryos

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

Primary Cell Cultures from Drosophila Gastrula Embryos

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

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

Purification of Transcripts and Metabolites from Drosophila Heads

For the last decade, we have tried to understand the molecular and cellular mechanisms of neuronal degeneration using Drosophila as a model organism. Although fruit flies provide obvious experimental advantages, research on neurodegenerative diseases has mostly relied on traditional techniques, including genetic interaction, histology, immunofluorescence, and protein biochemistry. These techniques are effective for mechanistic, hypothesis-driven studies, which lead to a detailed understanding of the role of single genes in well-defined biological problems. However, neurodegenerative diseases are highly complex and affect multiple cellular organelles and processes over time. The advent of new technologies and the omics age provides a unique opportunity to understand the global cellular perturbations underlying complex diseases. Flexible model organisms such as Drosophila are ideal for adapting these new technologies because of their strong annotation and high tractability. One challenge with these small animals, though, is the purification of enough informational molecules (DNA, mRNA, protein, metabolites) from highly relevant tissues such as fly brains. Other challenges consist of collecting large numbers of flies for experimental replicates (critical for statistical robustness) and developing consistent procedures for the purification of high-quality biological material. Here, we describe the procedures for collecting thousands of fly heads and the extraction of transcripts and metabolites to understand how global changes in gene expression and metabolism contribute to neurodegenerative diseases. These procedures are easily scalable and can be applied to the study of proteomic and epigenomic contributions to disease.

Purification of Transcripts and Metabolites from Drosophila Heads

We describe here the procedures for the extraction and purification of mRNA and metabolites from Drosophila heads. We are applying these techniques to better understand the cellular perturbations underlying neuronal degeneration. These methodologies can be easily scaled and adapted for other "omic" projects.

For the last decade, we have tried to understand the molecular and cellular mechanisms of neuronal degeneration using Drosophila as a model organism. ...

Organelle Transport in Cultured Drosophila Cells: S2 Cell Line and Primary Neurons.

Drosophila S2 cells plated on a coverslip in the presence of any actin-depolymerizing drug form long unbranched processes filled with uniformly polarized microtubules. Organelles move along these processes by microtubule motors. Easy maintenance, high sensitivity to RNAi-mediated protein knock-down and efficient procedure for creating stable cell lines make Drosophila S2 cells an ideal model system to study cargo transport by live imaging. The results obtained with S2 cells can be further applied to a more physiologically relevant system: axonal transport in primary neurons cultured from dissociated Drosophila embryos. Cultured neurons grow long neurites filled with bundled microtubules, very similar to S2 processes. Like in S2 cells, organelles in cultured neurons can be visualized by either organelle-specific fluorescent dyes or by using fluorescent organelle markers encoded by DNA injected into early embryos or expressed in transgenic flies. Therefore, organelle transport can be easily recorded in neurons cultured on glass coverslips using living imaging. Here we describe procedures for culturing and visualizing cargo transport in Drosophila S2 cells and primary neurons. We believe that these protocols make both systems accessible for labs studying cargo transport.

Organelle Transport in Cultured Drosophila Cells: S2 Cell Line and Primary Neurons.

Drosophila S2 cells and cultured neurons are great systems for imaging of motor-driven organelle transport in vivo. Here we describe detailed protocols for culturing both cell types, their imaging and analysis of transport.

Drosophila S2 cells plated on a coverslip in the presence of any actin-depolymerizing drug form long unbranched processes filled with uniformly polarized ...

Thawing, Culturing, and Cryopreserving Drosophila Cell Lines

Summary

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Chapters in this video

Primary Neuronal Cultures from the Brains of Late Stage Drosophila Pupae

Preparation of Neuronal Cultures from Midgastrula Stage Drosophila Embryos

Freezing, Thawing, and Packaging Cells for Transport

Medium-scale Preparation of Drosophila Embryo Extracts for Proteomic Experiments

Primordial Germ Cell Cryopreservation and Revival of Drosophila Strains

A Cell-based Assay to Investigate Non-muscle Myosin II Contractility via the Folded-gastrulation Signaling Pathway in Drosophila S2R+ Cells

Novel And Efficient Method for Drosophila Heart Fluorescence Staining with Cryosectioning

Primary Cell Cultures from Drosophila Gastrula Embryos

Purification of Transcripts and Metabolites from Drosophila Heads

Organelle Transport in Cultured Drosophila Cells: S2 Cell Line and Primary Neurons.