Materials and Reagents

1. Nunc^TM Thermanox^TM coverslips (Fisher Scientific, catalog number: 174942)

2. Flystuff embryo collection cage-mini, fits 35 mm Petri dishes (Genesee Scientific, catalog number: 59-105)

3. Fisherbrand^TM dissecting needle wood (Fisher Scientific, catalog number: 13-820-024)

4. Double-sided tape (Scientific Industries, catalog number: SI1616)

5. Nunc^TM cell culture/Petri dishes (Fisher Scientific, catalog number: 12-565-90)

6. Nunc^TM square BioAssay dishes (Fisher Scientific, catalog number: 166508)

7. Flystuff mesh basket, small, 3/4 inch inside diameter (Genesee Scientific, catalog number: 46-101)

8. Flystuff Nitex nylon mesh 630 μm, 45 inch wide roll, 1 foot/unit (Genesee Scientific, catalog number: 57-101)

9. Dechorionation chamber, prepared by adding a suitable size of Flystuff nylon mesh to the Flystuff mesh basket

10. Agar powder (Fisher Scientific, catalog number: A10752.22)

11. Sucrose (crystalline/certified ACS) (Fisher Scientific, catalog number: S5-500)

12. Apple/grape juice (any commercial product available from local sources)

13. Yeast granules (any commercial product available from local sources)

14. Methyl 4-hydroxybenzoate, 99% (Fisher Scientific, catalog number: AAA1428930)

15. Sodium hypochlorite solution (commercial bleach), available chlorine 4% (Fisher Scientific, catalog number: Q27908)

16. N-heptane, certified AR for analysis (Fisher Scientific, catalog number: H/0160/15)

17. Halocarbon oil 27 (Sigma-Aldrich, catalog number: H8773

18. Ultra-soft tissues (Kleenex)

Fly stocks

1. Duf-Gal4 (a gift from K. Vijayraghavan, NCBS, India)

2. M6-GapGFP [lines were created as part of a previous study (Aradhya et al., 2015)]

3. UAS-mCD8-mCherry (Bloomington Drosophila Stock Center, stock number: BL27391)

   Note: All stocks should be maintained at 25°C on standard Drosophila food medium.

Equipment

1. Drosophila incubator (Percival, catalog number: DR-36VL)

2. P10 micropipette (Eppendorf, catalog number: 3123000020)

3. Stereo dissecting microscope (Olympus Stereo Microscope System, catalog number: SZX7)

4. Leica TCS SP5 confocal microscope

Software

1. Imaris (BitPlane), https://imaris.oxinst.com/

2. Fiji (ImageJ), https://imagej.net/software/fiji/downloads

Procedure

1. Drosophila cage setup, embryo collection, and dechorionation

   1. Set up a cross between the M6-gapGFP, Duf-Gal4, and UAS-mCD8-mCherry transgenic flies with 40–60 flies in an embryo collection cage of suitable size (Figure 2A).

   2. Prepare apple/grape juice agar medium using methyl 4-hydroxybenzoate according to standard protocols (Cold Spring Harb Protoc, 2011), pour it into 35 mm cell culture dishes, and allow the food medium to solidify at room temperature. The plates with medium can be stored at 4°C for up to two weeks (Figure 2A).

   3. Add a layer of yeast paste to the center of the apple juice agar plate before setting up the cage to stimulate the egg production.

   4. Allow the flies to mate and start laying eggs in the egg-laying cage for two days in a 25°C incubator with a 12:12 h light/dark cycle.

   5. Once the flies are synchronized to the cage, the apple juice agar plates can be changed every 12 h to collect embryos with a developmental time point ranging from 0 to 12 h. Alternatively, collect the egg-laying plates by transferring flies to a new egg collection cage every 2 h and incubate separately in a 25°C Drosophila incubator to obtain age-synchronized embryos.

   6. Wash the embryos from the plates with a fine brush into a dechorionation chamber; rinse with water repeatedly to remove any traces of yeast paste (Figure 2B–D).

   7. Dechorionate embryos using 50% commercial bleach with continuous swirling of the dechorionation chamber for up to 2 min, until all embryos look like shiny rice granules. At this step, embryos can be observed under the dissection microscope to ensure proper removal of the chorion membrane (Figure 2E).

   8. Thoroughly rinse the dechorionation chamber with distilled water to remove any traces of bleach; pat dry the embryos by placing the nylon mesh from the dechorionation chamber on a pile of Kleenex tissues for a few minutes (Figure 2F).

   9. Dechorionated embryos are hygroscopic in nature and tend to stick to each other. After pat drying for 2–3 min, gently pick up the clusters of embryos with a fine brush or dissecting needle; place them on a rectangular block of apple juice agar cut from the square cell culture plates containing a uniform layer of apple/grape juice agar medium (Figure 2G–H).




2. Embryo alignment and picking onto a coverslip

   10. Align the embryos in a linear fashion on the edge of the rectangular agar block. Maintain the orientation of the embryos in such a way that the dorsal side faces the edge of the agar block, and the lateral side faces up to visualize the abdominal AMPs (Figure 2I). For other specific tissues or cells, the embryos can be aligned accordingly so they can be visualized easily using an inverted microscope.

   11. Place approximately 10 strips of double-sided tape (10 × 1 cm) in a 100 mL glass bottle and fill it with 90 mL of N-heptane. Allow the tape and heptane mixture to sit at room temperature for 12 h for proper extraction of the glue. The heptane/glue solution can be kept at 4 °C and used for several experiments.

   12. Using a P10 micropipette, add a small volume of heptane/glue solution to the center of a rectangular coverslip in a thin line that covers the entire coverslip length (Figure 2J).

   13. Allow the glue to semidry for 5 min in a sterile empty plastic box.

   14. Gently press the side containing glue against the aligned embryos on the agar block; this way, the embryos are transferred to the coverslip in the same alignment of the agar block, with the lateral side facing towards the coverslip (Figure 2K). This side can be easily visualized with high magnification lenses, which require applying immersion oil to the coverslip.

   15. Cover the embryos with a thin layer of halocarbon oil 27 to prevent them from desiccation (Figure 2L). Halocarbon oil allows embryos to exchange gases with the surrounding air, keeping them in healthy conditions for a long period.




3. Imaging the embryos with a confocal microscope using time-lapse series

   16. Visualize the embryos using an inverted microscope, in which the objectives can touch the bottom side of the coverslip without disturbing the embryos (Figure 2M). Place the coverslips in the microscope in the same manner as glass slides using suitable holders.

   17. Using the lower magnification eyepiece of a Leica SP5 confocal microscope with time series imaging, select suitable embryos with appropriate developmental stage and better visualization of muscle stem cells and surrounding tissues (Figure 2N).

   18. Use the 40× oil immersion objective for enlargement of particular hemisegments of the embryo and better observation of the tissues of interest. Select Z-stacks based on the depth of tissue needed to be imaged (Figure 2O).

   19. Using the Fiji (ImageJ) software, analyze the raw files from the confocal microscope and generate images with the Z-stack of the selected optical section.

   20. Using Imaris (BitPlane) software, perform 3D reconstruction of both single time-point image and time-series live imaging.

Data analysis

1. For maximum intensity projection of the single time-point image, select the desired optical sections in ImageJ and export them as a Z-stack picture.

2. Similarly, use the Imaris software to generate a 3D rotating model of either a single time-point projection or images captured on a time-lapse series mode.

Figure 1. Dual-color live imaging of muscle stem cells and surrounding tissues. (A) Lateral view of stage 15 Drosophila M6-GapGFP; Duf-Gal4 X UAS-mCD8-mCherry embryos; AMPs expressing GFP are in green and the differentiated muscles expressing mCherry are in red. Scale bar: 100 μm. (B) Two hemisegments around the lateral muscles and associated AMPs have been magnified to observe the ultrastructure of cytoplasmic extensions protruding from AMPs. Scale bar: 9 μm.

Acknowledgments

This protocol was adapted from the previously published paper (Aradhya et al., 2015). We thank Pierre Pouchin for helping in the image processing during the initial analysis. We also thank the Imaging platform at GReD institute, France for allowing us to use the Leica SP5 confocal microscope.

Competing interests

The authors declare no competing interests.

References

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