Use of Immunolabeling to Analyze Stable, Dynamic, and Nascent Microtubules in the Zebrafish Embryo

Summary

Immunolabeling methods to analyze distinct populations of microtubules in the developing zebrafish brain are described here, which are broadly applicable to other tissues. The first protocol outlines an optimized method for immunolabeling stable and dynamic microtubules. The second protocol provides a method to image and quantify nascent microtubules specifically.

Abstract

Microtubules (MTs) are dynamic and fragile structures that are challenging to image in vivo, particularly in vertebrate embryos. Immunolabeling methods are described here to analyze distinct populations of MTs in the developing neural tube of the zebrafish embryo. While the focus is on neural tissue, this methodology is broadly applicable to other tissues. The procedures are optimized for early to mid-somitogenesis-stage embryos (1 somite to 12 somites), however they can be adapted to a range of other stages with relatively minor adjustments. The first protocol provides a method to assess the spatial distribution of stable and dynamic MTs and perform a quantitative analysis of these populations with image-processing software. This approach complements existing tools to image microtubule dynamics and distribution in real-time, using transgenic lines or transient expression of tagged constructs. Indeed, such tools are very useful, however they do not readily distinguish between dynamic and stable MTs. The ability to image and analyze these distinct microtubule populations has important implications for understanding mechanisms underlying cell polarization and morphogenesis. The second protocol outlines a technique to analyze nascent MTs specifically. This is accomplished by capturing the de novo growth properties of MTs over time, following microtubule depolymerization with the drug nocodazole and a recovery period after drug washout. This technique has not yet been applied to the study of MTs in zebrafish embryos, but is a valuable assay for investigating the in vivo function of proteins implicated in microtubule assembly.

Introduction

Microtubules (MTs) are polymers of α- and β-tubulin that assemble into linear protofilaments, several of which combine to form a hollow tube^1,2. MTs are polarized structures, with fast-growing plus ends and slow-growing minus ends that are anchored at the centrosome or other microtubule-organizing center (MTOC)³. De novo MT formation is initiated by nucleation at the γ-tubulin ring complex (γ-TURC), which provides a template for MT assembly⁴. In any given cell, two populations of MTs can be distinguished that turn over at different rates. Dynamic MTs explore their cellular environment by switching between phases of growth and shrinkage in a process known as dynamic instability⁵. Unlike dynamic MTs, stable MTs are non-growing and have a longer half-life than dynamic MTs⁶.

Decades of research in cell biology has provided a sophisticated array of tools to study MT structure and function and resulted in a large body of knowledge on these cytoskeletal elements. For instance, MTs play a central role in the establishment and maintenance of cell polarity, which is attributable not only to their intrinsic polarity, but also to the differential subcellular distribution of stable versus dynamic MTs^7,8. In contrast, far less is understood about MT architecture and function in more complex three-dimensional (3-D) environments, such as the vertebrate embryo, in part due to the challenge of imaging the MT cytoskeleton at high resolution. Despite this limitation, the recent generation of GFP-expressing transgenic lines that label MTs or transient expression of fluorescently-tagged MT markers has increased our understanding of the dynamic changes that MTs undergo and their cellular and developmental role in the zebrafish embryo. The entire MT network can be imaged in transgenic lines in which tubulin is either directly labeled⁹ or tubulin polymers are indirectly labeled using MT-associated proteins Doublecortin-like-kinase (Dclk) or Ensconsin (EMTB)^10,11. Other lines (and constructs) have been generated that enable assessment of MT intrinsic polarity by specifically labeling MT plus ends or centrosome-anchored minus ends^11,12,13,14. The power of these tools lies in the ability to study MT dynamics in live, developing organisms. Such studies have revealed, for example, the spatial and dynamic distribution of MTs in specific cell populations, the orientation of mitotic spindles in tissues undergoing morphogenesis (an indicator of the plane of cell division), the polarity of the MT polymer as it relates to processes such as cell elongation and migration, and MT growth rate determined by comet speed^9,13,15. The limitation of these tools is that they do not readily discriminate between stable and dynamic MT populations.

Drawing from the rich cell biology literature, immunolabeling methods to image stable and dynamic MTs in the zebrafish embryo are described here, which are complementary to the use of transgenic lines. The widespread use of such immunolabeling methods in the zebrafish has been somewhat hampered by the difficulty in preserving MT integrity during the fixation procedure. Protocol 1 outlines an optimized method for immunolabeling total, dynamic, and stable MTs in cross sections of the developing zebrafish hindbrain. Furthermore, a straightforward method using commercially available software is described to quantify these MT populations. Stable MTs are distinguished from dynamic MTs based on several post-translational modifications of α-tubulin, such as acetylation and detyrosination, which accumulate on stable MTs over time^16,17. In the zebrafish embryo, acetylation occurs on ciliary and axonal MTs but not on stable interphase MTs¹⁸, limiting the usefulness of this marker to a subset of stabilized MTs. In contrast, detyrosination appears to occur on all stable MTs in the zebrafish embryo¹⁸. This post-translational modification exposes the carboxy-terminal glutamic acid of α-tubulin (detyrosinated tubulin)¹⁸ and can be detected using anti-Glu-tubulin¹⁹. Although detyrosination occurs preferentially on stable MTs, experimental evidence indicates that this post-translational modification is a result of, rather than a cause of, MT stability¹⁶. The reciprocal MT population, composed of dynamic MTs, is distinguished using an antibody, anti-Tyr-tubulin, that specifically recognizes the tyrosinated form of α-tubulin¹⁹. Following immunolabeling with these markers and confocal imaging, the quantitative analysis of MTs (length, number, and relative abundance) can be performed in defined regions of the developing neural tube. A streamlined method is provided here for performing this analysis using 3-D image-processing software. This method can be applied to address questions regarding morphogenesis and the establishment or maturation of cell polarity²⁰. Indeed, the elaboration of polarized arrays of stable MTs accompanies many developmental events, including photoreceptor morphogenesis²¹, epithelialization of cells in the developing neural tube¹⁸ and axon formation⁸.

Protocol 2 describes an in vivo adaptation of a cell biology assay to analyze MTs during their assembly phase (nucleation/anchorage and growth)^22,23. Nascent MTs are nucleated at the centrosome and subsequently anchored to subdistal appendages of the mother centriole²³. A method to analyze nascent MT regrowth following depolymerization is described. This protocol provides details on the nocodazole treatment to depolymerize MTs, the drug washout procedure and the post-treatment recovery period. MT re-growth is monitored at regular intervals post washout by immunolabeling with markers for total MTs (anti β-tubulin) alongside markers for the centrosome (anti γ-tubulin) and nucleus (4',6-diamidino-2-phenylindole (DAPI)), according to the general procedures described in Protocol 1. The MT depolymerization step of this protocol is essential as it enables assessment of de novo MT growth rather than extension of preexisting MTs. This technique is therefore distinct from other published procedures to measure MT growth rates (in absence of depolymerization) by using a plus tip marker such as end binding protein 3 fused to green fluorescent protein (EB3-GFP), as shown in Tran et al., 2012¹¹. Furthermore, this assay is particularly useful for analyzing embryos defective in de novo MT assembly, such as the previously reported NEDD1 mutants in which recruitment of γ-tubulin to the centrosome is impaired, resulting in incomplete neural tube formation and neuronal defects²⁴.

Protocol

Ethics Statement: The procedures described below follow the University of Maryland Baltimore County animal care guidelines.

1. Analysis of Stable and Dynamic MTs Using Immunolabeling (Protocol 1)

1. Manual dechorionation of embryos prior to fixation
   1. Obtain freshly spawned embryos by pouring off excess system water and then collecting remaining embryos into a plastic Petri dish (refer to Table of Materials).
   2. Remove any debris from the system water and transfer embryos to a new dish filled with embryo medium (refer to Table of Materials) to ensure that the embryos develop in a clean environment.
   3. Allow the embryos to develop to the desired stage in a temperature-controlled incubator at 28.5 °C.
   4. Place embryos younger than 24 h post-fertilization (hpf) in a glass dish prior to dechorionation.
      NOTE: Dechorionate embryos prior to fixation to maximize rapid penetration of the fixative and preserve MT integrity. Use embryo medium instead of system water to provide the additional Ca²⁺ required during dechorionation.
   5. Manually remove the chorions from embryos while in Petri dish, using fine forceps under a dissecting microscope.
      1. Pinch a small area in the round, transparent chorion that encircles the embryo with a pair of forceps and gently pull forceps apart to create a rupture in the membrane.
      2. Enlarge the opening by delicately prying on the ruptured chorion using forceps. Be careful not to touch the embryo with the forceps as it could rupture.
2. Fixation of staged embryos
   1. Transfer staged, dechorionated embryos to 1.5 mL centrifuge tubes. Remove as much embryo medium as possible using a glass Pasteur pipette.
      NOTE: Perform fixation and drug treatments on young (mid-somitogenesis) embryos, prior to the formation of the neural centers mediating pain sensation, which require no additonal procedure to alleviate pain during euthanasia. Developmental stages are as defined in Kimmel et al., 1995²⁵. The 4-5 and 11-12 somite stages were used to obtain images for Figures 2 and 3.
   2. Prepare 4% paraformaldehyde (PFA)/MT assembly buffer (MAB) fixative (refer to Table of Materials) by combining 1 mL 8% PFA per 1 mL 2X MAB and adding 2 µL 100% Triton X-100 per 1 mL of total volume.
      CAUTION: Wear gloves while handling solutions containing PFA and Triton X-100, which are skin irritants.
   3. Fix embryos in 1 mL 4% PFA/MAB fixative for 5 min at 28.5 °C. Aspirate the fixative with a pipette, replace it with 1 mL fresh fixative, and incubate for 3 h at room temperature (RT) on a rocker.
      NOTE: Samples must be fixed quickly at their biological temperature (28.5 °C for zebrafish) to prevent temperature-dependent MT depolymerization.
3. Aspirate fixative and add 1 mL 1x Tris-buffered saline with NP40 (TBS-NP40) buffer. Gently agitate at RT on a rocker three times for 5 min each. Store embryos at 4 °C in 1 mL fresh 1X TBS-NP40 for no more than 7 days.
   CAUTION: Wear gloves when handling solutions containing NP-40, a skin irritant.
4. Sectioning embryos for immunolabeling
   1. Heat RT 4% low melting point (LMP) agarose embedding medium in a closed container until the solution becomes clear using a hot plate set to 50 °C positioned close to a dissecting microscope. Keep the container closed between samples and heated throughout the embedding process (steps 1.4.4-1.4.6).
   2. Transfer embryos from the 1.5 mL centrifuge tubes to a Petri dish using a glass pipette and fill it with 1X TBS-NP40.
   3. Remove the large yolk cells from somitogenesis stage embryos (4-5 and 11-12 somites) in the Petri dish using fine forceps under the magnification of a dissecting microscope²⁶. Hold the embryo by the tail bud with one pair of forceps and peel away the yolk cells with the other pair in order to preserve the hindbrain tissue. Transfer the de-yolked embryos to an area of the Petri dish free of yolk debris.
      NOTE: Embed embryos in the agarose-filled mold individually to prevent premature hardening of the LMP agarose.
   4. Fill one 12 mm x 5 mm x 3 mm well of the sectioning mold with 200 µL melted LMP agarose using a micropipette. Perform the steps 1.4.5.-1.4.6. quickly (within 20 s of filling the mold) to embed embryo before the LMP agarose cools to RT and solidifies.
   5. Use fine forceps to transfer a de-yolked embryo by the tailbud from the Petri dish to the agarose-filled mold toward its tapered end under a dissecting microscope.
   6. Use fine forceps to orient the embryo into the mold such that the vibratome cuts in the desired plane. Create transverse sections by orienting the embryo such that the hindbrain tissue runs parallel to the length of the mold with its dorsal surface facing the edge and its anterior surface facing the tapered region end. Repeat steps 1.4.4-1.4.6 for the remaining embryos.
   7. Allow the agarose embedding to solidify for 5 min at RT.
   8. Generate 40 µm sections of the tallest axis of the agarose embedded embryos (steps 1.4.1-1.4.7) using a vibratome with the sectioning dish filled with 1x TBS-NP40. Transfer sections of interest to a 24-well plate in 500 µL 1x TBS-NP40 using fine forceps. Place the sections of only one embryo per well.
      NOTE: Refer to reference¹⁸ for more details. Ensure that sections remain hydrated at all times in at least 250 µL of buffer and rock at low speed (10-25 rpm) for remaining steps to prevent separation from agarose embedding. Detergents present in the blocking and wash solutions should reduce the surface tension of the liquid medium and allow submersion of the sections. Check that sections remain in the wells during and after all manipulations. Use caution to prevent accidentally discarding sections during washes.
5. Remove the buffer and add 500 µL of blocking solution. Rock for at least 1 h at RT.
   NOTE: Use a blocking solution that contains 5% sera from the host species of each secondary antibody to be used (refer to Table of Materials).
6. Incubate in 300 µL primary antibodies diluted in blocking buffer for 36-72 h at 4 °C on a rocker. Wash twice in 600 µL 1x TBS-NP40 on a rocker for 30 min each, at RT.
   NOTE: Double-label sections by incubating in primary antibodies against total MTs (anti β-tubulin, or anti α-tubulin) and stable MTs (anti-Glu-tubulin) or dynamic MTs (anti-Tyr tubulin). Select primary antibodies that have been raised in different host species when double labeling for total and post-translationally modified α-tubulin populations. Refer to Table of Materials for antibody dilutions.
7. Incubate in 300 µL of fluorophore-conjugated secondary antibodies diluted in blocking buffer on a rocker for 16-24 h, at 4 °C in the dark. Wash twice in 600 µL 1x TBS-NP40 on a rocker for 30 min each, at RT.
   NOTE: Wrap the multi-well dish containing secondary antibody in foil from this point onwards and after each manipulation to prevent quenching. Select secondary antibodies that react with the host immunoglobulin of the primary antibody. Choose secondary antibody fluorophores that have separate, non-overlapping emission spectra. Refer to Table of Materials for antibody dilutions.
8. Incubate the embryos in 500 µL of DAPI solution on a rocker for 30 min, at RT. Wash three times in TBS-NP40 rocking at RT for 5 min each.
   NOTE: Nuclear labeling provides cellular context for the MT quantification performed in step 1.12.
9. Place a drop of mounting medium with anti-fade agent on the center of a dust-free slide. Use fine forceps to transfer sections to the mounting medium droplet. Place a dust-free coverslip on top of the sample. Store slides in a dry, dark, and cool place, wrapped in foil, until imaging is performed.
   NOTE: Circling the sections on the back of the slide using a fine-tipped permanent marker prior to imaging will help to identify sections when using the microscope.
10. Confocal Imaging
    1. Mount sections on an inverted laser scanning confocal microscope by affixing the slide to the stage with the coverslip facing the objective. Determine the appropriate optics (objective, laser, and channel settings such as gain and offset) on a control slide and keep them consistent between samples²⁷. Avoid oversaturating the pixels to prevent data loss.
    2. Capture Z-stacks confocal images using channel settings for the selected secondary antibody fluorophores and save the image files²⁷. Acquire Z-stacks for each section.
       NOTE: Replicate the parameters used to acquire the images in Figures 2 and 3 by using the following acquisition settings: mode = XYZ; objective magnification = 63X oil immersion lens; objective numerical aperture = 1.4; Z-step = 0.1 µm; Z-depth = 16.23 µm. Use the following channel settings: DAPI excitation with 20% UV-range laser, emission filter range = 430-480 nm, photomultiplier (PMT) gain = 525 V, and PMT offset = -1.72%; 448 nm fluorophore (refer to Table of Materials) excitation with 20% 488 nm laser, emission filter range = 493-573 nm, PMT gain = 689 V, and PMT offset = -0.2%; 594 nm fluorophore excitation with 32% 594 nm laser, emission filter range = 608-706 nm, PMT gain = 768 V, and PMT offset = -6.8%.
    3. Save raw data files with unique, descriptive file names and create a copy for editing in image analysis software.
11. Compilation of Z-stacks for displaying maximum projections
    1. Open the data file copy using public domain 3-D image analysis software (e.g., ImageJ). Check that each channel appears as an individual image sequence (Z-stacks).
    2. Split image channels by using the following menu sequence : “Images/Color/Split channels”.
    3. Create a merged image by overlaying the channels of interest by using the following menu sequence: "Images/Color/Merge channels." Select the 594 nm, 488 nm, and DAPI channels to be false colored red, green, and blue, respectively. Check "Create composite" and select "OK"²⁸.
       NOTE: Omit the DAPI channel to better convey detail specific to MTs in a maximum projection as in Figure 2 and 3, by only selecting false colors for the other two channels.
    4. Examine the merged Z-stack and make note of the beginning and ending positions of the inner best Z-planes for all visible channels. Dismiss the outer Z-planes that typically have suboptimal signal due to the uneven surfaces of the section. Refer to reference²⁹ for details.
    5. Visualize the merged Z-stack as a single 2-D image by performing a maximum intensity projection of the Z-stack using the following 3-D image analysis menu sequence: "Images/Stack/Z-project." Enter the starting and ending positions of the inner best Z-planes from step 1.11.3 as the "Start slice" and "Stop slice," respectively. Select "Max intensity" as the projection type and click "OK". Refer to reference²⁸ for more details.
12. Analyzing MT labeling
    1. Open the commercial 3-D image analysis software. Select "Create Library" and provide a descriptive name for the image library. Click "Create." Drag raw image files generated from the confocal microscope into the library. Larger files require more time to transfer.
    2. Select a file to analyze. Choose "Extended Focus" from the "view" menu to display the channel-merged image in the main window.
    3. Adjust the thresholding by dragging the slider tool for each channel to the left or right until the background signal is reduced and the true signal is robust. Observe that each channel shows a true signal for the molecule labeled (e.g., DAPI channel showing oblong or mitotic nuclei but not auto-fluorescence from the cytoplasm or agarose).
    4. Select the "Freehand Region of Interest (ROI)" tool and outline the region of interest to be analyzed. Select the "Actions" tab followed by "Crop to Selection" to crop the image. Save the cropped image file under a new name. Click the "Measurements" tab to create the protocol for filtering specific objects relevant to the 3-D analysis.
    5. Drag "Find Objects" to the protocol window. Rename the first protocol "DAPI." Select the DAPI channel in the dropdown menu. Drag the following settings to the DAPI protocol and place them below "Find Objects" in the following order (Table 1): "Fill Holes in Objects"; "Separate Touching Objects"; "Exclude Objects by Size"; "Exclude Not Touching ROIs".
       NOTE: The goal of the settings in Table 1 are to first set a threshold that discards signals whose distribution and size are inconsistent with the size of objects being analyzed. For example, eliminate a signal not large enough to be a nucleus when counting nuclei.
    6. Perform the sequence (step 1.12.9) to assemble the remaining filters for β-tubulin and other markers using the settings in Table 1.
    7. Select "Measure" at the bottom of each protocol. Choose "Intensity and Volume Measurement" and "Skeletal Length" for all tubulin labeling, but only the former for the DAPI signal.
    8. Draw an ROI around the region to be measured. Observe the measurements under the "Summary" tab after the software processes the region. Copy the data and save them to a workable spreadsheet, as in Table 2. Create a back-up copy of the spreadsheet for later analysis.
    9. Select measurements of interest (for example, length of MT bundle, number of MT bundles/nucleus, as revealed with different markers) in the spreadsheet and analyze to determine the averages for each group.
       NOTE: The average MT bundle length = the sum of the 'mean skeletal length for β-tubulin' for each embryo divided by the total number of embryos. Refer to row 20 of Table 2. Format the spreadsheet so that variables and experimental groups are easily graphed.

2. De Novo MT Assembly Assay (Protocol 2)

1. Construct and test the multi-well flow-through apparatus (Figure 1) 2 days prior to the experiment.
   NOTE: The apparatus enables simultaneous washout of multiple experimental groups following nocodazole treatment using supplies from Table of Materials. Silicone sealer requires at least 24 h of drying time before it poses no toxicity risk to the embryos.
   1. Split a 50 mL centrifuge tube in half lengthwise, using a jig or band saw.
   2. Cut 7 semi-circles, with a radius of 3 cm, out of 70 µm nylon mesh and trim them to fit tightly into one half of the split centrifuge tube. Glue the semi-circles into the centrifuge tube parallel to the 10 mL gradation markings using aquarium-safe silicon sealer. Allow the device to dry for 2 days and rinse by soaking in a beaker of water for 2-3 h.
   3. Line the top (threaded) end of the cut centrifuge tube with modeling clay such that the height of the liquid retained in the flow-through device has a depth of ¼ inch (Figure 1, views 2 and 3).
   4. Prepare the washout apparatus by removing the plunger from a 50-mL syringe and inserting 12 inches of fine tubing into the tip. Push the tubing in as far as it will go and seal around the joint using modeling clay.
   5. Pre-wet the mesh using embryo medium to allow the liquid to run through the entire flow-through device. Angle the device on ice so that liquid pools in all compartments but still empties out the front where the clay rim is located. Using a ring stand, suspend the washout apparatus above the flow-through device on ice (Figure 1).
   6. Chill 200 mL of embryo medium on ice and pour enough into the washout apparatus to ensure that all air bubbles are cleared and that the flow rate is approximately 7 mL/min. Adjust the flow rate by changing the height of the syringe.
2. Enzymatically dechorionate embryos
   1. Make a working solution of non-specific protease by diluting 1 mL of 10 mg/mL non-specific protease stock in 20 mL embryo medium.
   2. Perform chemical dechorionation on embryos 1 h prior to the timepoint when they are expected to reach the desired developmental stage. Digest chorions by removing embryo medium from 100 mm Petri dishes containing staged embryos and adding 20 mL of non-specific protease working solution.
   3. Incubate embryos at 37 °C for 5 min.
      NOTE: Do not exceed 5 min or use a higher concentration of non-specific protease solution, as this will result in the embryos falling apart once treated with nocodazole.
   4. Quickly pipette out non-specific protease and refill dishes with approximately 25 mL embryo medium. Repeat once.
   5. Using a 1-mL glass pipette, transfer embryos younger than 24 hpf to glass dishes to protect them from damage.
   6. Complete dechorionation by manually removing chorions using a pair of fine forceps, as described in step 1.1.5.
   7. Place glass Petri dishes containing dechorionated embryos in a 28.5 °C incubator for a minimum of 30 min until they reach the desired developmental stage.
3. Depolymerize the existing MTs
   1. Prepare a working solution of 5 µg/mL nocodazole by combining 50 µL 1 mg/mL stock nocodazole with 10 mL ice cold embryo medium.
      CAUTION: Use gloves when handling nocodazole, a skin irritant.
   2. Exchange the embryo medium of the nocodazole treatment group with 10 mL cold nocodazole working solution. Place Petri dishes on ice for an appropriate time for the developmental stage (for example, 1 h for 4-5 somite embryos). Set aside untreated control embryos in a Petri dish on ice to be fixed alongside washout samples in step 2.3.4.1.
   3. Transfer embryos using a fire polished 1-mL glass pipette to the flow-through apparatus, using separate compartments for each experimental group. Start the nocodazole washout by pouring ice cold embryo medium into the top of the 50 mL syringe.
      NOTE: Use at least 30 embryos per experimental group. Experimental groups could consist of control embryos or a variety of morpholino or RNA-injected embryos. The washout will require a total of about 150 mL of embryo medium to be added every 8-10 min. Washout the nocodazole while continuing to inhibit MT growth with ice. Keeping the embryos on ice is essential for the success of this assay because MTs are unstable at cold temperatures and cold delays the development in early embryos.
   4. Allow MTs to regrow after 20 min of washout at RT by transferring embryos to glass Petri dishes containing warm (28.5 °C) embryo medium using a fire polished 1 mL glass pipette. As soon as the embryos are transferred, start a timer.
      1. Fix the control and washout embryos at 1 min, 5 min and 10 min by pipetting approximately 10 embryos into a 1.5 mL centrifuge tube filled with 1 mL 4% PFA/MAB fix (28.5 °C) and following the directions in step 1.2.3.
4. Prepare samples for immunolabeling as described in sections 1.3-1.5.
5. Immunolabel floating sections and image embryos as described in sections 1.6-1.10 with the following changes to primary antibody specifications: use 1:500 rabbit anti-γ-tubulin and 1:200 mouse anti-β-tubulin.
6. Process and analyze images using 3-D image analysis software, as described in step 1.12.

Results

Analysis of stable and dynamic MTs using immunolabeling
In Protocol 1, the distribution of MT sub-populations during early (neural keel) and late (neural rod) stages of neural tube development is revealed, using Glu-tubulin and Tyr-tubulin as markers for stable and dynamic MTs, respectively. Dynamic MTs predominate in the hindbrain at the neural keel stage (4-5 somites) (Figure 2A-D). As the keel develops...

Discussion

There are currently many methods for imaging MT dynamics in early zebrafish development, ranging from live imaging of tagged molecules to immunolabeling of fixed tissue^11,12,13,14. Although MTs in a single cell can exist in either dynamic or stable states, epithelialization is a process in which MTs are progressively stabilized over time. Using markers for stable and dynamic MTs offers a way to...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Agarose			Used to treat petridishes.   Prepare 1% agarose by heating a solution of  1 gram agarose per 100 ml 1X embryo medium in a microwave until polymerized.
Kpipes	Sigma	P7643
NaCl	Sigma	S7653
Tris-HCl	Sigma	T3253-500G
KCl	Sigma	P9333-500G
CaCl2·2H2O	Sigma	C5080
NP-40	American Bioanalyticals	AB01424
EGTA	Sigma	E3889-25G
MgCl2	Sigma	M2670-500G
Bovine serum albumin (BSA)	Fisher	BP1605
Triton-x	American Bioanalyticals	AB02025
Anti-Fade mounting medium	Invitrogen	P10144
Mouse anti-β-tubulin	Developmental studies Hybridoma Bank	E7	1/200
Rabbit anti-γ-tubulin	Genetex	GTX113286	1/500
Rabbit anti-α-tubulin	Genetex	GTX108784	1/1000*
Rabbit anti-detyrosinated-tubulin	Millipore	AB3201	1/200-1/1000*  Titrate antibody with first use of new lot.
Rabbit anti-tyrosinated-tubulin	Millipore	ABT171	1/500
Mouse anti-centrin	Millipore	04-1624	1/1000
Goat 488 anti-rabbit	Thermofisher	A11008	1/500
Goat 594 anti-rabbit	Thermofisher	A11012	1/500
Goat 594 anti-mouse	Thermofisher	A11005	1/500
Goat 488 anti-mouse	Thermofisher	A11001	1/500
Vibratome	Vibratome	1500
Forceps	World Precision Instruments	555227F
100 mm petri dish	Cell treat	229693
35 mm petri dish	Cell treat	229638
50 ml falcon tube	Fisher	14-432-22
Woven nylon mesh 70 um	Amazon.com	B0043D1SZG
Micropipette	Gilson	F123602
Glass pipette	Fisher	NC-999363-9
Aquarium sealant	Amazon.com, by MarineLand	Silicone Sealer 1 oz (Tube)
Ring stand	Fisher	14-675BO
Microbore PTFE Tubing, 0.022"ID	Cole-Parmer	WU-06417-21
Modeling clay	Amazon.com	Sargent Art 22-4000	Any wax or oil based non-toxic modeling clay will suffice
Clamp	Fisher	02-215-466
60ml syringe	Fisher	14-820-11
Embryo medium (E3)			34.8 g NaCl 1.6 g KCl 5.8 g CaCl2·2H2O 9.78 g MgCl2·6H2O To prepare a 60X stock, dissolve the ingredients in H2O, to a final volume of 2 L. Adjust the pH to 7.2 with NaOH. Autoclave. To prepare 1X medium, dilute 16.5 mL of the 60X stock to 1 L.
Blocking Solution			50 ml TBS-NP-40 2.5 ml normal goat serum 1 g BSA 625 µl Triton-X
TBS-NP-40 (pH 7.6)			155 mM NaCl 10 mM Tris HCl 0.1% NP-40
2x MAB (pH6.4)			160 mM KPIPES 10 mM EGTA 2 mM MgCl2
Commercial 3-D Image processing Software	PerkinElmer	Volocity (V 6.2)
Dry block heater	VWR	12621-108	Used as a hot plate to melt agarose in Protocol 1.
Dissecting Microscope	Leica	MZ12
Confocal Microscope	Leica	SP5
Flat embedding mold	emsdiasum.com	BEEM 70904-01
Public domain image processing software	NIH	ImageJ (V 1.5)
* Success varies by lot number