Sequential Photo-bleaching to Delineate Single Schwann Cells at the Neuromuscular Junction

Podsumowanie

Visualizing individual cells in densely packed tissues, such as terminal Schwann cells (SCs) at neuromuscular junctions (NMJs), is challenging. "Sequential photo-bleaching" allows delineating single terminal SCs, for instance in the triangularis sterni muscle explant, a convenient nerve-muscle preparation, where sequential bleaching can be combined with time-lapse imaging and post-hoc immunostainings.

Streszczenie

Sequential photo-bleaching provides a non-invasive way to label individual SCs at the NMJ. The NMJ is the largest synapse of the mammalian nervous system and has served as guiding model to study synaptic structure and function. In mouse NMJs motor axon terminals form pretzel-like contact sites with muscle fibers. The motor axon and its terminal are sheathed by SCs. Over the past decades, several transgenic mice have been generated to visualize motor neurons and SCs, for example Thy1-XFP¹ and Plp-GFP mice², respectively.

Along motor axons, myelinating axonal SCs are arranged in non-overlapping internodes, separated by nodes of Ranvier, to enable saltatory action potential propagation. In contrast, terminal SCs at the synapse are specialized glial cells, which monitor and promote neurotransmission, digest debris and guide regenerating axons. NMJs are tightly covered by up to half a dozen non-myelinating terminal SCs - these, however, cannot be individually resolved by light microscopy, as they are in direct membrane contact³.

Several approaches exist to individually visualize terminal SCs. None of these are flawless, though. For instance, dye filling, where single cells are impaled with a dye-filled microelectrode, requires destroying a labelled cell before filling a second one. This is not compatible with subsequent time-lapse recordings³. Multi-spectral "Brainbow" labeling of SCs has been achieved by using combinatorial expression of fluorescent proteins⁴. However, this technique requires combining several transgenes and is limited by the expression pattern of the promoters used. In the future, expression of "photo-switchable" proteins in SCs might be yet another alternative⁵. Here we present sequential photo-bleaching, where single cells are bleached, and their image obtained by subtraction. We believe that this approach - due to its ease and versatility - represents a lasting addition to the neuroscientist's technology palette, especially as it can be used in vivo and transferred to others cell types, anatomical sites or species⁶.

In the following protocol, we detail the application of sequential bleaching and subsequent confocal time-lapse microscopy to terminal SCs in triangularis sterni muscle explants. This thin, superficial and easily dissected nerve-muscle preparation^7,8 has proven useful for studies of NMJ development, physiology and pathology⁹. Finally, we explain how the triangularis sterni muscle is prepared after fixation to perform correlated high-resolution confocal imaging, immunohistochemistry or ultrastructural examinations.

Protokół

1. Triangularis Sterni Explant (Figure 1)

Timing: 15 min.

1. Prepare surgical instruments: 2 pairs of forceps, 1 pair of scissors, 1 pair of spring scissors, 1 tissue culture dish (10-cm). Pre-bubbled (minimum for 15 min) cooled (4 °C) Ringer's solution with 5% CO₂/ 95% O₂. Fill 15-cm tissue culture dish with ice and cover it with metal plate. Prepare dissection microscope and place the 15-cm dish with ice under the dissection scope in order to cool the explant during dissection.
2. Lethally anesthetize the mouse by isoflurane overdose (or any other approved method of sacrifice). Spray the mouse with 70% ethanol to prevent fur contamination of the explant. For SC bleaching, we used Plp-GFP mice, which can be crossed to Thy1-OFP3 or Thy1-Membow13 for simultaneous visualization of the axon.
3. Using the pair of large scissors, make a midline incision of the skin over the sternum and two incisions parallel to the lower edge of the rib cage.
4. Using the pair of large scissors, remove the skin, open the abdominal wall, and make incisions parallel to the rib cage all the way back to the vertebral column. Then dissect off the pectoral muscles by making incisions close to the muscle insertion at the sternum.
5. Cut the diaphragm open just below the xiphoid cartilage and dissect off the diaphragm along its costal insertions.
6. Holding the rib cage by the xiphoid process with a set of forceps, start cutting the ribs off the vertebral column, as close as possible to their insertions. The left and right cuts should converge above the heart towards the manubrium sterni. Try to avoid cutting major blood vessels (especially the subclavian veins). Better visibility is achieved by gently lifting the preparation while holding onto the xiphoid process with forceps.
7. Make a transverse cut just below the manubrium sterni and transfer the explant into the 10-cm dish with cooled 5% CO₂/ 95% O₂-bubbled Ringer's solution. Place the 10-cm dish on the metal plate covering the 15-cm tissue culture dish filled with ice. All further steps should be done under the dissection microscope.
8. Using small spring scissors remove the remnants of thymus, pleura, diaphragm (inside) and pectoral muscles (outside; Figure 1B-D).
9. To fit the explant to the 3.5-cm dish, dissect off all the ribs that do not insert to the sternum. This is best done using small spring scissors and cutting the tissue in between ribs (Figure 1E).
10. Pin the triangularis sterni nerve-muscle explant into the Sylgard coated 3.5-cm tissue culture dish using minutien pins (shortened to < 4 mm; Figure 1G). Two pins should go through cartilaginous (white) parts of the sternum. Insert at least two pins through the ribs both on the left and right side of the explant aiming for the softer cartilaginous parts and avoiding the ribs under or close to the triangularis muscle. The more pins are used, the better (we typically use 8-10). As you pin down the preparation, make sure that the ribs are somewhat spread, fixing the muscle into a slightly stretched position.
11. Optional: Visualize synaptic sites containing acetylcholine receptors by adding bungarotoxin coupled to Alexa dyes (concentration of 0.8 μg/ml in 5% CO₂/ 95% O₂-bubbled Ringer's solution). Incubate pinned explant in Sylgard coated dish for 15-20 min at room temperature then wash several times with 5% CO₂/ 95% O₂-bubbled Ringer's solution.

2. Bleaching SCs and Optional Time-lapse Microscopy (Figure 2)

Timing: 30 - 45 min + optional 1 - 5 hr for time lapse.

1. Transfer 3.5-cm Sylgard-coated dish to a confocal microscope equipped with an argon laser (488 nm wavelength) and water immersion objectives (4x, 0.13 NA; 20x, 0.5 NA and 100x, 1.0 NA or 60x, 0.9 NA).
2. Optional for time-lapse microscopy: Insert 3.5-cm Sylgard-coated dish into heating ring, install superfusion system and temperature probe (Figure 2A). Make sure that none of them touch the explant, the rim of the dish or the Sylgard coating. Heat the sample to 33-35 °C. For SC bleaching without time-lapse, room temperature is better, as cells show less dynamics between bleaching steps.
3. With a 4x air objective observe innervation pattern of triangularis sterni muscle and find triangularis sterni endplate band. Switch to 20x dipping-cone objective and start looking for superficial regions within the endplate band (areas overlying ribs are good candidates). Change objective to 100x or 60x dipping-cone objective to check on individual NMJs. Ideal is an NMJ that is covered by several SCs and is located very superficially (Figure 2B). If you perform time-lapse imaging after bleaching, select up to 3 NMJs that are relatively close together to increase yield.
4. Acquire a confocal image of the NMJ before photo-bleaching individual SCs (Figure 2B). (For full resolution imaging, e.g. on an Olympus FV1000 microscope, use a 100x, 1.0 NA objective and 2.5 zoom, which results in Nyquist-limited sampling of ~0.1 μm per pixel.)
5. "Park" the 488 nm laser beam centrally on the nucleus of a SC using maximal power for 5 seconds (alternatively an efficient scan pattern in a small region of interest can be used, such as the "tornado scan" function on an Olympus microscope; as we use a confocal microscope, the laser is focussed into the image-conjugate planes and hence, at 488 nm with an objective of 1.0 N.A., < 0.5 μm in diameter). Re-focus on the cell and judge bleaching result. If necessary repeat bleaching step again until GFP levels are reduced to near-background levels. Acquire an image after bleaching (Figure 2C). It is critical to make sure that the bleached region is outside of any overlap between two cells - if there is overlap, bleaching in a second cell will be obvious.
6. Repeat step above until all but one SC are bleached (Figure 2D-E). The last "unbleached" SC is suitable for confocal time-lapse microscopy. Reconstruct single cells by subtraction of images, e.g. using Photoshop software, to delineate single SC morphology and territory (Figure 2F). Be aware that subtracting two mages adds noise (e.g. by importing them in consecutive "layers" in Photoshop and then setting the top channel to "difference" in the drop down menu at the top of the channels tab). This can be circumvented by using the "despeckle" function on the channels before subtraction and cropping away any background that obviously does not originate from the bleached cell. To optimize contrast, it can be necessary to adjust the brightness of the two channels in the "levels" window. The resulting image of the bleached cell is the superimposed on the original image of a synapse, pseudo-colored in a unique hue and made transparent to color the territory of the bleached cell in the original image (from doing this for all bleached and the last, unbleached cells the image shown in Figure 2F results).
7. Optional: Start confocal time-lapse microscopy after bleaching all but one SCs. Take an image at fixed intervals (for example every 5 to 10 min). Use as little laser power as possible. Up to 3 NMJs can be imaged at the same session.
8. Make a map of the time-lapsed NMJs by taking an image at 100x without zoom, then images of the region using 20x and 4x objectives (Figure 2G-I). This "map" is needed to find NMJs following immunohistochemistry of a fixed muscle.
9. For image processing, convert individual images into maximum intensity projections and save in tiff format. Combine all z-projected time-points into a stack and align in xy, e.g. using the "stackreg" plugin¹⁰ in Fiji (a package based on the open source software ImageJ; National Institutes of Health).

3. Fixation and Immunohistochemistry (Figure 3)

Timing: Overnight.

1. Transfer the explant into a 50-ml reaction tube containing at least 15 ml 4% PFA by carefully removing the pins. Post-fix the anterior thoracic wall containing the triangularis sterni muscle for 1 hr on ice. Rinse fixed tissue with 0.1 M glycine in PBS (to quench residual fixative and hence reduce background) for at least 10 min. Samples can be stored at this point and processed later.
2. Transfer fixed explant to a 10-cm Sylgard coated tissue culture dish filled with 0.01 M PBS. Cut out a trapezoid shape with one side parallel to the sternum and the other through the bone-to-cartilage transitions - this contains the triangularis muscle on its surface. Remove lower ribs with a horizontal (i.e. trans-sternal) cut so that the caudal end of the triangularis muscle can be freely accessed (Figure 3A-D).
3. Insert a hypodermic needle as a pin into the upper part of the trapezoid (Figure 3E). Use a hypodermic needle attached to a 1 ml syringe and forceps to remove the triangularis muscle on the surface by gently holding onto a caudal corner of the muscle and using the needle as a micro-scalpel. Make sure that cuts are made parallel to the plane of the thoracic wall. Once the caudal part of the muscle is released, insert another hypodermic needle as a pin below the muscle through the thoracic wall - this immobilizes the preparation and allows exerting a gentle pull on the muscle using forceps (Figure 3F). As you are cutting connective tissue insertions, "peel" away the muscle from the thorax. Cut last caudal attachment with spring scissors. Remove fat and blood vessel remnants using forceps. Be careful not to rip away the nerves. Note: Use separate sets of tools and dishes for working with live and fixed tissue.
4. Start immunohistochemistry (using a standard protocol) by transferring tissue samples into blocking solution for 1 hr on a shaker at room temperature. Smallest possible volume for staining is 200 μl using a 96-well plate.
5. Apply primary antibody diluted in blocking solution, 200 μl per well, overnight at 4 °C on a shaker.
6. Wash in 0.01 M PBS three times for 10 min.
7. Apply suitable secondary antibody for 1-2 hr at room temperature diluted in blocking solution.
8. Wash in 0.01 M PBS three times for 10 min.
9. Mount in anti-fading medium (e.g. Vectashield) and coverslip.
10. Place slide on magnetic metal plate, place magnet on top of the sample to flatten for a few hours or overnight at 4 °C. Seal with nail polish.

Wyniki

An example of a triangularis sterni explant ready for imaging dish is shown in Figure 1G. This explant is particularly suitable for imaging NMJs ex vivo as the triangularis muscle consists only of a few layers of muscle fibers. This allows obtaining high resolution images from explants derived from transgenic mouse lines that highlight either SCs (Plp-GFP²) and/or axons (Thy1-XFP¹). Critical factors for high quality imaging include: (i) avoiding touching t...

Dyskusje

The SC bleaching method presented here is simple, fast and versatile: (i) It enables revealing single SC morphology and dynamics by confocal microscopy based on a single transgene - which is a significant advantage when combining the approach e.g. with disease models that require additional alleles. (ii) The method is rapid, as from dissection to fixation it can be performed in half a day. (iii) The number of applications is broad, as it can be combined with other methods, such as cell ablations, imaging organel...

Materiały

Name	Company	Catalog Number	Comments
70% (vol/vol) ethanol solution	Roth	T913.1	in spray bottle
isoflurane	Forene, Abbott		any other approved anaesthetic can be used for lethal anaesthesia
transgenic mice (Plp-GFP)			to be obtained from cited sources
dissection microscope with cold-light illumination	Olympus SZ51		equipped with Schott KL 1500 LCD
forceps #2	Fine Science Tools	11233-20
forceps #5	Fine Science Tools	11295-00
scissors, large medical	Fine Science Tools	14108-09
scissors, small angled spring	Fine Science Tools	15033-09
in-line heater	Warner Instruments	SF-28
heating ring for 3.5-cm dishes	Warner Instruments	64-0110 DH-35
two channel temperature control system	Warner Instruments	TC-344B
superfusion pump system			custom-built
15-cm tissue culture dish	Sarstedt	83.1803.003	filled with ice and covered by metal plate
10-cm tissue culture dish	Sarstedt	83.1802.003	with oxygenated Ringer's solution
3.5-cm tissue culture dish	Sarstedt	83.1800.003	filled with Sylgard polymer
Sylgard polymer	Dow Corning	Sylgard 184 Silicone Elastomer Kit
confocal microscope	Olympus	FV1000	with argon laser
50-ml reaction tube	Sarstedt	62.547.254 PP
4% PFA in PBS	Sigma	P6148
cannula 0.5 mm x 25 mm	Neolab	E-1510
syringe 1 ml	Neolab	E-1496
synaptophysin antibody	Invitrogen	18-0130	rabbit
secondary antibody	Invitrogen	A-11012	Alexa 594
24-well plate	Sarstedt	83.1836
0.01 M PBS	Sigma	P4417
0.1 M glycine in PBS	Roth	3790.1
coverslips	Neolab	E-4132
slides	Neolab	E-4121
Vectashield	Vector labs	H-1000
minutien pins ×10	Fine Science Tools	26002-20	shortened to < 4 mm
α-Bungarotoxin coupled to Alexa 594	Invitrogen (Molecular Probes)	B-13423
Blocking Solution
0.01 M PBS
0.2% Triton-X100	Roth	3051.3
10% Normal Goat Serum	Abcam	ab7481
1% bovine serum albumin	Sigma	A7030
Ringer bubbled with 95% O2 /5% CO2
125 mM NaCl	Sigma	S7653
2.5 mM KCl	Sigma	P9333
1.25 mM NaH2PO4	Sigma	S8282
26 mM NaHCO3	Sigma	S6297
2 mM CaCl2	Sigma	21114
1 mM MgCl2	Sigma	63020
20 mM glucose	Sigma	G7528
Table 1. Specific reagents and equipments.