Visualization of Motor Axon Navigation and Quantification of Axon Arborization In Mouse Embryos Using Light Sheet Fluorescence Microscopy

Summary

Here, we describe a protocol for visualizing motor neuron projection and axon arborization in transgenic Hb9::GFP mouse embryos. After immunostaining for motor neurons, we used light sheet fluorescence microscopy to image embryos for subsequent quantitative analysis. This protocol is applicable to other neuron navigation processes in the central nervous system.

Abstract

Spinal motor neurons (MNs) extend their axons to communicate with their innervating targets, thereby controlling movement and complex tasks in vertebrates. Thus, it is critical to uncover the molecular mechanisms of how motor axons navigate to, arborize, and innervate their peripheral muscle targets during development and degeneration. Although transgenic Hb9::GFP mouse lines have long served to visualize motor axon trajectories during embryonic development, detailed descriptions of the full spectrum of axon terminal arborization remain incomplete due to the pattern complexity and limitations of current optical microscopy. Here, we describe an improved protocol that combines light sheet fluorescence microscopy (LSFM) and robust image analysis to qualitatively and quantitatively visualize developing motor axons. This system can be easily adopted to cross genetic mutants or MN disease models with Hb9::GFP lines, revealing novel molecular mechanisms that lead to defects in motor axon navigation and arborization.

Introduction

Spinal MNs are the part of the central nervous system but innervate peripheral muscles to control movement. In the developing spinal cord, MN progenitors (pMNs) are established according to the signals emanating from the notochord and adjacent somites. All differentiated post-mitotic MNs are then generated from pMNs, eventually giving rise to a series of MN subtypes along the rostrocaudal axis of the spinal cord^1,2. Spinal MNs are topographically and anatomically well organized. Their morphological arrangement correlates with the position of their respective target in the periphery³. Upon reaching their muscle targets, axons receive cellular and exogenous neurotrophic factors that induce them to extend and branch further into muscles. Innervation and branching defects may contribute to the failure to form neuromuscular junctions (NMJ). For example, glial-derived neurotrophic factors (GDNF)-induced Pea3 is indispensable for axon arborization into cutaneous maximus (CM) and latissimus dorsi (LD) muscles^4,5. In addition, DINE knockout mouse embryos show defective arborization of phrenic nerves in the diaphragm, causing respiratory failure and mortality immediately after birth^6,7. Therefore, this last step of MN maturation (i.e., axonal projection and branching) is critical to ensure communication between neurons and target cells.

To view arborization patterns, researchers normally conduct confocal imaging or two-photon fluorescence light microscopy of sectioned or whole-mount samples^8,9,10. Both of these microscopy techniques generate acceptable resolution and depth penetration. Two-photon fluorescence light microscopy involves excitation of fluorophores by simultaneous absorption of two lower-energy photons¹¹. Since two-photon excitation uses near-infrared radiation, the decreased excitation frequency contributes to reduced scattering and better tissue penetration up to 1 mm in tissue, thus allowing imaging with greater depth. Confocal microscopy removes by filters the out-of-focus signals and only collects light within the focal plane¹². With this approach, images of samples from different focal planes can be combined to produce a three-dimensional (3D) image via a Z-stack function. Nevertheless, signal intensity is reduced as most of the light is blocked and high numerical apertures obscure the depth-of-field. More importantly, both techniques contribute to the severe photodamage and phototoxicity since the whole specimen receives illumination even when only one plane is imaged at a given time.

To circumvent these shortcomings, LSFM has become a favored alternative, with the advantages of being fast, light-efficient, and less phototoxic^13,14. In addition, LSFM allows multi-view imaging. This approach is particularly suited to visualizing motor axons and their dispersing terminals as they spread through 3D space. LSFM outperforms the other two options because samples are mounted on a stage that allows rotation around a vertical axis and movements along the x, y, and z axes. This set-up not only allows for a minimally blocked view of the sample but also the choice of a desirable illumination path, a shortcoming of two-photon and confocal microscopy, both of which require mounting of samples on a flat slide. Therefore, LSFM is the most suitable tool for 3D imaging of axon arborization and for quantification of motor nerve terminals in mouse embryos.

Protocol

All of the live animals were kept in a specific pathogen free (SPF) animal facility, approved and overseen by IACUC of Academia Sinica.

1. Fixation

1. Collect embryos of embryonic day 12.5 (E12.5) then decapitate and eviscerate them.
2. Fix the embryos individually in 24-well plates with 1 mL/well of freshly prepared 4% paraformaldehyde in 1x phosphate buffer saline (PBS) overnight. Incubate at 4 °C on a shaker.
3. Wash the fixed embryos at least 3x, each for 5-10 min, with 1 mL of 1x PBS and incubate overnight at 4 °C on a shaker to remove the residual paraformaldehyde.

2. Whole-mount Immunostaining

1. Permeabilize each embryo in 1 mL of 0.5% PBS-Triton-X-100 (PBST) overnight at 4 °C on a shaker.
2. Block each sample with 1 mL of 10% FBS prepared in 1x PBS overnight at 4 °C on a shaker.
3. Incubate the embryo with 1 mL of anti-GFP primary antibody (1:1,000 dilution in 10% FBS) at 4 °C for 72 h with constant shaking to intensify the GFP signal of motor nerves.
4. After the primary antibody incubation, wash with 1 mL of 0.5% PBST over the course of 1-2 days at 4 °C on a shaker, changing the 0.5% PBST at least three times.
5. Apply 1 mL of secondary antibody (1:1,000 dilution in 10% FBS) and incubate overnight in the dark at 4 °C with constant shaking.
6. Wash 3x with 1 mL of 0.5% PBST at 4 °C on a shaker over the course of 2-3 days. Keep samples in 1x PBS at 4 °C until the day before imaging.
   NOTE: Embryos can be dissected into smaller segments before clearing, depending on which part of the embryos will be imaged. Forelimbs are preserved in this experimental approach (Figure 1A).
7. Incubate the embryo in a commercial clearing reagent with a refractive index of 1.49 nD in a 1.5 mL tube, protected from light at room temperature overnight, to render the embryo transparent for imaging.
   NOTE: The volume of the clearing reagent is approximately five times that of the sample volume.

3. LSFM (2–3 h)

1. Sample set-up
   1. Set up 5X/0.1 illumination optics and 5X/0.16 detection optics. Assemble the sample holder and sample capillary (1.5 mm internal diameter, green) and place them into the microscope.
      NOTE: Refer to the microscope's Operating Manual for detailed set-up procedures.
   2. Mount the embryo as follows:
      1. Prepare the P200 pipette tip by cutting away the upper part so that it fits the diameter of the capillary and remove the pointed part (~ 3 mm) for the sample attachment.
      2. Melt the blunted end of the pipette tip using a small flame.
      3. Extinguish the flame and quickly attach the embryo vertically onto the melted end.
      4. Fit the upper part of the pipette tip with the sample capillary.
   3. Allow the chamber buffer to equilibrate with the embryo for 1 min to clear off debris or bubbles.
   4. Using the imaging software, select Locate capillary under the Locate tab and adjust the x, y, z axes to position the sample capillary.
   5. Select Locate sample and zoom to 0.6X to focus on the embryo. Rotate the embryo to ensure that the long axis of the imaged limb aligns with the light path of the two light sources (Figure 1B).
2. Image acquisition
   1. Under the Acquisition tab, define the light path parameters such as detection objectives, laser blocking filter, beam splitter, cameras, and lasers.
      NOTE: The GFP channel is used in this experiment (Excitation wavelength: 488 nm; emission filter: BP 505 to 545 nm, beam splitter: SPS LP 560).
   2. Check the pivot scan checkbox for shadow reduction.
   3. Define the acquisition settings: bit depth, 16 bit; zoom, 0.36-0.7X; single-side illumination (left/right) or dual-side illumination.
   4. Click Continuous and set the laser intensity, exposure time, laser power, and light sheet position to acquire sharper images.
      NOTE: The laser power is kept as low as possible to minimize photodamage.
   5. Press STOP to end image acquisition.
3. Multidimensional acquisition
   1. Define the z-stack by moving the Z position for the first and last image. Click Optimal to set the slice number.
   2. Click Start Experiment to acquire the selected z-stack.
   3. When it is done, save the image in .czi format.
4. Image processing (optional)
   1. Proceed with Dual side fusion under the Lightsheet Processing channel if dual-side illumination is applied. Multiview processing is necessary if multi-views are acquired to combine images from multiple angles.
   2. Create a 2D image using data from the highest intensity pixels along the projection axis under the Maximum Intensity Projection channel.
   3. Under Copy channel, click Subset to select subsets of images from the original set.

4. Quantification of Axon Arborization (30 Min for Each Individual Nerve)

1. Open the image file in the imaging analysis software (by default, the image containing the XYZ data is opened in Surpass mode and as a 3D-rendered view).
2. Adjust the image color, brightness, and contrast using the Display Adjustment window (Edit | Show Display Adjustment) to detect filaments based on local intensity contrast.
3. Click on the Add New Filaments icon and select the Autopath (no loop) algorithm in the drop-down menu.
4. Select the region of interest (in this case, the segmenting axon of interest). Click Next when finished.
5. Define the starting and seed points by assigning the largest and thinnest diameter measurements, which can be measured using the Slice mode.
6. Assign a starting point at the edge of the region of interest. To achieve manual addition or removal of starting points, first change the pointer mode (Navigate | Select) and then Shift + right-click at the points of interest.
7. Select manual thresholds for seed points to ensure that all of the visible arborization is marked. Change the pointer mode (Navigate | Select) and then Shift + left-click at the points of interest to manually add or remove seed points.
   NOTE: It is important to manually remove background noises and signals from neighboring nerves.
8. Check the box Remove seed points around starting points.
9. Check Remove disconnected segments to allow exclusion of points that are too far away and that may represent background noise. Indicate the Maximum Gap Length in the next step to define the upper limit for exclusion.
10. Adjust the threshold for background subtraction, which uses a Gaussian filter to estimate the background intensity of every voxel.
11. Set automatic threshold for dendrite diameter using the Approximate cross-section area algorithm.
12. Skip the steps for spine calculation.
13. Finish the process and choose the desired style and color.
14. Uncheck the volume box in Properties to view only the reconstructed axons.
15. Under the Statistics tab, select Detailed. Use Filament No. Dendrite Terminal Points to quantify the motor nerve terminals as an indicator of motor axon arborization.
    NOTE: Statistical annotation can be added if desired.
16. Export the image of the reconstructed axon as a .tif file.

Results

LSFM provides detailed 3D visualization of MN trajectory and axon arborization in mouse embryos. Under bright field, tissues appear completely transparent after being immersed in the commercial clearing reagent. No shrinkage or swelling of the sample was noticed after up to one week of storage in clearing reagent before imaging. Under fluorescence channel, motor neurons are labeled with transgenically expressed GFP (Movie 1). In some instance, details of the axon structur...

Discussion

Several steps in the protocol may be subjected to changes under certain circumstances. For example, the duration of fixation depends on the age of the embryos, varying from 2 h to 1 or more days using freshly-made paraformaldehyde. Since fixation is carried out prior to whole mount immunostaining, for antibodies that are sensitive to protein crosslinking, methanol can be used as an alternative fixative agent. For a high signal-to-noise ratio upon staining, it is necessary to optimize the detergent concentration (between ...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Hb9::GFP	The Jackson labortory	005029	Collect embryos of embryonic day 12.5 (E12.5)
4% Paraformaldehyde (PFA)			For 200ml: Add 20ml 10X PBS, 8g PFA in ddH2O. Adjust pH to 7.4 with NaOH (10N). Filter sterilize and store at -20 °C.
Phosphate buffer saline 10X (PBS 10X)			For 1L: Add 80 g NaCl, 2 g KCl,14.4g Na2HPO4, 2.4 g KH2PO4 and top up with ddH2O. Autoclave and store at RT.
Triton X-100	Sigma	X100-500ML
Fetal Bovine Serum	ThermoFisher	26140079
Sheep polyclonal anti-GFP	AbD Serotec	4745-1051	1:1000
Alexa Fluor 488 donkey anti-sheep	Invitrogen	A-11015	1:1000
RapiClear 1.49 clearing reagent	SunJin Lab	RC149001
1.5ml micro tube	Sarstedt	72.690.001
24 wells plate	ThermoFisher	142475
5 SA Tweezer	ideal-tek	3480641
Iris Scissors striaght sharp/sharp	Aesculap	BC110R
Microsurgery Scalpels, single use	Aesculap	BA365
Dissecting microscope	Nikon	SMZ800
Shaker	TKS	RS-01
Lightsheet Z.1 microscope	Carl Zeiss Microscopy
Imaris 8.4.0 image analysis software	Bitplane, Zurich, Switzerland
B6.Cg-Tg(Hlxb9-GFP)1Tmj/J (Hb9::GFP mice)	The Jackson Laboratory	005029