Visualization of Endosome Dynamics in Living Nerve Terminals with Four-dimensional Fluorescence Imaging

Summary

Four-dimensional (4D) imaging is utilized to study the behavior and interactions among two types of endosomes in living vertebrate nerve terminals. Movement of these small structures is characterized in three dimensions, permitting confirmation of events such as endosome fusion and exocytosis.

Abstract

Four-dimensional (4D) light imaging has been used to study behavior of small structures within motor nerve terminals of the thin transversus abdominis muscle of the garter snake. Raw data comprises time-lapse sequences of 3D z-stacks. Each stack contains 4-20 images acquired with epifluorescence optics at focal planes separated by 400-1,500 nm. Steps in the acquisition of image stacks, such as adjustment of focus, switching of excitation wavelengths, and operation of the digital camera, are automated as much as possible to maximize image rate and minimize tissue damage from light exposure. After acquisition, a set of image stacks is deconvolved to improve spatial resolution, converted to the desired 3D format, and used to create a 4D "movie" that is suitable for variety of computer-based analyses, depending upon the experimental data sought. One application is study of the dynamic behavior of two classes of endosomes found in nerve terminals-macroendosomes (MEs) and acidic endosomes (AEs)-whose sizes (200-800 nm for both types) are at or near the diffraction limit. Access to 3D information at each time point provides several advantages over conventional time-lapse imaging. In particular, size and velocity of movement of structures can be quantified over time without loss of sharp focus. Examples of data from 4D imaging reveal that MEs approach the plasma membrane and disappear, suggesting that they are exocytosed rather than simply moving vertically away from a single plane of focus. Also revealed is putative fusion of MEs and AEs, by visualization of overlap between the two dye-containing structures as viewed in each three orthogonal projections.

Introduction

Time-lapse imaging of living tissue provides visual access to dynamical structure-function relations that cannot be appreciated in fixed or living preparations imaged at a single point in time. Often, however, the tradeoff for access to temporal information is a decrease in optical resolution. High numerical aperture oil-immersion objectives are impractical in living tissue because of their narrow range of focus, leaving water immersion or dry objectives as the only alternatives. Moreover, the increased resolution afforded by confocal optics cannot be utilized in some living preparations due to phototoxicity from the relatively high levels of illumination required^1,2. Lastly, while several real-time or time-lapse optical techniques are available that offer enhanced resolution, their applicability is limited to preparations where structures of interest can be positioned within a few hundred nanometers of the objective¹. The method described makes use of relatively low-cost equipment, is versatile, yet offers improved resolution compared to more commonly-used time-lapse techniques. It is intended for use in individual laboratories as well as imaging facilities.

The method utilizes conventional epifluorescence microscopy, combined with a sensitive digital camera and with hardware designed to rapidly acquire sets of images at slightly different focal planes (z-stacks). Each z-stack is digitally deconvolved to increase resolution. One feature of 3D time-lapse (4D) imaging is precise tracking of moving organelles or other structures. When properly set up, imaged structures do not go out of focus, and movement in all three directions can be observed and quantified. Thus it is impossible for a stained structure to disappear over one or more time-lapse frames merely by drifting above or below a narrow focal plane. The method also serves as a sensitive tool for assessing the interactions and possible fusion of small structures. Conventional epifluorescence or confocal images of structures near the diffraction limit (a few hundred nm) do not confirm fusion even if merged images show overlap of their respective labels³. Fusion is suggested, but it remains possible that the objects are separated horizontally or vertically by a distance that is below the diffraction limit. Three- or four-dimensional imaging, in contrast, permits viewing the objects in each of three orthogonal directions. The appearance of fusion in all three views increases the level of certainty. And, in some living preparations, directed or Brownian movement of putatively fused objects provides further proof when both labels move together in time. Of course, when near the diffraction limit the level of certainty in discerning structures from background, or showing that they contain two dyes (fusion), is not absolute. If applicable, specialized techniques, such as fluorescence resonance energy transfer (FRET)⁴, are more appropriate.

Protocol

1. Stain the Preparation with Supravital Dyes

1. For the garter snake dissection protocol see Stewart et al.⁵ and Teng et al.⁶ Reptilian tissue remains physiological for longer times, and with less bacterial contamination, when kept at low temperatures (see below). Mammalian tissue is usually maintained at room temperature or higher.
2. For lysosomal vital dye staining, dissolve the dye in cold reptilian Ringers solution 1:5,000 (0.2 μM). Incubate at 4 °C for 15 min. Wash several times with cold Ringers. Image as soon as possible.
3. For FM1-43 staining using KCl stimulation, dilute the dye in high-KCl Ringers 1:500 (7 μM). Incubate at 4 °C for 30-60 sec maximum. Wash quickly three times with cold Ringers, ~1 min/rinse. Image as soon as possible.
4. For FM1-43 staining using hypertonic (sucrose) stimulation, dilute the dye in 0.5 M sucrose Ringers as above. Incubate at 4 °C for 2-5 min. Wash as in step 1.3 above with cold Ringers. Image as soon as possible.
5. For FM1-43 staining via electrical stimulation, see Teng et al.⁶ Briefly, the preparation is placed a dish containing physiological saline solution and the dye. The nerve is stimulated with a preprogrammed train of 200 μsec rectangular pulses ( ~7 V, 30 Hz, 18 μsec). Wash as in step 1.3 above with cold Ringers. Image as soon as possible.

2. Configure the Preparation for Imaging

1. Orient the preparation so that structures of interest are as close as possible to the microscope objective.
2. If an inverted microscope is used, utilize a chamber whose bottom contains a thin round cover slip. Typically, the imaging chamber should have a thin stainless steel bottom with a 25 mm diameter #1 thickness glass cover slip at the center. If an upright microscope is used, a bottom coverslip is not required but is useful to permit imaging with transmitted light (e.g. differential interference contrast, DIC) to orient the specimen and locate objects of interest.
3. Choose an appropriate objective to obtain the highest possible 3D resolution. There are tradeoffs among numerical aperture (n.a.), working distance, magnification, and type of lens (dry, water- and oil-immersion). For thin preparations like tissue cultures, oil objectives are best. Using an upright microscope, float a cover slip on the aqueous bath, and use immersion oil between the top of the cover slip and the objective.
4. If deconvolution software is used, the vendor might provide predetermined point spread functions (PSFs) for certain objectives. If no such information is provided, or if an unsupported objective is chosen, determine the PSF by imaging fluorescent microdots or similar diffraction-limited objects^7,8.

3. Establish the Desired Depth of Field and Number of Images Desired per Time-lapse Frame

1. Select the total depth of field so that moving or interacting structures of interest do not disappear or go out of focus as they move in the z-direction. The z-field should slightly exceed the vertical dimension of the cell or cell process being imaged. For vertebrate motor terminals, 15-20 µm is typical.
2. Calculate the z-axis step needed for each increment of focus. Resolution along the z-axis varies depending upon properties of the objective; it is about one-fourth of the x-y plane resolution. If either confocal imaging or deconvolution software is used, z-axis resolution is improved. Improve final resolution by deliberate oversampling in the z-direction ⁵, but see also step 3.3 below. A typical step interval is in the range from 400-1,500 nm for 40-100X objectives. Light should be shuttered off between each z-step image.
3. Select the number of images per z-stack, namely the desired depth of field divided by the step interval. Time to complete a typical z-stack is 1-10 sec. Fast-moving objects (100 nm/sec) can appear blurred in a 3D image stack because each image plane corresponds to a slightly different time point. Also, each additional image contributes to photobleaching and possible phototoxicity (see Discussion). If either situation pertains, choose a larger z-step to collect fewer images per stack. Compensate later using image interpolation software (step 6.3 below).

4. Select the Time-lapse Frame Rate

Choose by experimentation a rate that is just adequate to smoothly resolve changes with time such as movement, interactions or fusion events⁹. Under sampling can produce motion artifacts (sampling errors), while oversampling unnecessarily increases exposure to light. Collect either a single long sequence or several repeated sequences from the same preparation, each with a relatively small total time interval (e.g. 10 time points x 30 sec interval = 5 min). If possible, view the preparation with continuous epifluorescence illumination to roughly estimate movement velocities, including drift of the entire preparation if present.

5. Complete All Live Imaging for a Particular Preparation

Reptilian preparations typically remain robust for ~1-2 hr, longer if cooled.

6. Analyze Data According to Desired Use

1. Retain all raw data files. While digital storage is usually not a problem, processing time is significant even with fast personal computers or workstations. For this reason, crop images into a region of interest [ROI]. Assure that the entire region of interest is in the cropped window during the entire time course.
2. Deconvolve image stacks using appropriate software and the correct point spread function. Confirm that resolution is improved and that no artifact has been generated by the deconvolution algorithm. Figure 3 shows example images.
3. Use an interpolation algorithm to expand z-axis apparent resolution. A 6X expansion from an actual 1.5 μm image plane separation to an apparent 0.25 μm separation is suggested. Alternatively, use some combination of oversampling (step 3.2) and interpolation.
4. Perform contrast, brightness, noise filtering, photobleaching and other typical image processing adjustments if desired. Image manipulation standards dictate that for most scientific work, it is appropriate that the same corrections be applied to all images, both within a stack and at different time points. The consequence of a particular adjustment should be assessed among all images ⁹.
5. Select a particular display mode for export of data. The most straightforward display is stereo video using either red-green or red-blue anaglyphs (examples in Figure 3), stereo pairs, or alternating left/right eye frames with shutter glasses. Anaglyphs are limited to single-color. Enhance apparent image depth if desired to improve z-axis visual resolution.
6. Experiment with various filtering and image enhancement techniques. For example, Laplacian filtering is useful to increase contrast of small structures above background. The brightness of pixels at the center of a running window is enhanced while brightness of surrounding areas is reduced. Note that some filtering methods do not work well in combination.
7. Apply drift correction if there is substantial movement of the preparation over time. Such movement is common in living muscle, even with drugs added to suppress action potentials and synaptic potentials. A pixel registration algorithm (e.g. IMARIS, Adobe AfterEffects, TurboReg plugin for ImageJ) aligns time-lapse images and can reduce, but usually not completely eliminate, such motion.

Results

Data shown are from snake neuromuscular terminals (see low and high magnification views in Figure 3; the endocytic dye (FM1-43) uptake creates a haze that fills each bouton) and, in particular, macroendosomes (MEs) and acidic endosomes (AEs) within these terminals⁵. MEs are created by bulk endocytosis during neural activity¹⁰ and their number declines exponentially with time after activity has ceased⁶. Use of 4D live imaging was to determine if MEs move towards the plasma...

Discussion

The most critical aspect of 4D imaging is management of the duration and intensity of light exposure. Photobleaching decreases image signal-to-noise ratio and can be problematic or not depending on various factors, including choice of fluorophores. Nonspecific damage to living tissue (phototoxicity) is related to photobleaching, and can sometimes be identified using fluorescent probes designed for the purpose^2,12 or by examination of morphology with suitable brightfield optics, such as differential interferenc...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Equipment
SGC5	Biotium, Hayward, CA	70057	Final conc: 10 mM
FM1-43FX	Invitrogen, Carlsbad, CA	F35335	Final conc: 7 mM
LysoTracker Red	Invitrogen, Carlsbad, CA	L7528	Final conc: 0.2 mM
Reptilian Ringers pH 7.2
NaCl			145 mM
KCl			2.5 mM
CaCl2			3.6 mM
MgSO4			1.8 mM
KH2PO4 (Dibasic)			1.0 mM
HEPES			5.0 mM
High KCl Reptilian Ringers pH 7.2
NaCl			86 mM
KCl			60 mM
CaCl2			3.6 mM
MgSO4			1.8 mM
KH2PO4 (Dibasic)			1.0 mM
HEPES			5.0 mM
High Sucrose Ringers pH 7.2
NaCl			145 mM
KCl			2.5 mM
CaCl2			3.6 mM
MgSO4			1.8 mM
KH2PO4 (Dibasic)			1.0 mM
HEPES			5.0 mM
Sucrose			0.5 M (17.1 g/50 ml)
Axioplan 200 inverted microscope	Carl Zeiss, Thornwood, NY		www.zeiss.com
N-Achroplan 63X water objective; n.a.=0.9; Working distance=2.4 mm	Carl Zeiss, Thornwood, NY		www.zeiss.com
DG4 combination light source/excitation filterwheel switcher	Sutter Instruments, Novato, CA	175W Xenon arc lamp	www.sutter.com
Lambda 10-2  emission filterwheel switcher	Sutter Instruments, Novato, CA		www.sutter.com
Sensicam CCD camera	Cooke Instruments, Tonawanda, NY		www.cookecorp.com
Cascade 512 CCD camera	Photometrics, Tucson, AZ		www.photometrics.com
Imaging dishes- made in-house-11 cm dia.; 25 mm dia. #1 coverslip embedded; magnetic pins
Software
Slidebook 5.0	Intelligent Imaging Innovations, Denver, CO	Deconvolution; Drift correction;3D and 4D data presentation	www.intelligent-imaging.com
IMARIS 7.5.2	Bitplane, South Windsor, CT	Drift correction; 3D and 4D data presentation	www.bitplane.com
AfterEffects CS6	Adobe, San Jose, CA	Drift correction	www.adobe.com
ImageJ 1.46	National Institutes of Health, Bethesda, MD	Multiple plugins available; Stereo pair construction	http://rsbweb.nih.gov/ij
Zeiss LSM	Carl Zeiss, Thornwood, NY	Stereo pair construction	www.zeiss.com