The confocal microscope was purchased with funds from the U.S. National Science Foundation (NSF), grant #DBI-0722569. The research was supported by the U.S. National Institutes of Health/National Institute of General Medical Sciences (NIH/NIGMS) grant #GM085290 and U.S. Department of Defense (DOD) grant #W81XWH-16-1-0466 awarded to R.M. Brewster. E. Vital was supported by a grant to UMBC from the Howard Hughes Medical Institute through the Pre-college and Undergraduate Science Education Program, grant #52008090. S.P. Brown was supported by a U.S. Department of Education GAANN Fellowship, a Meyerhoff Graduate Fellowship funded by NIH/NIGMS grant #GM055036, and a Research Assistantship funded by the U.S. DOD grant #W81XWH-16-1-0466.

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The authors have nothing to disclose.

There are currently many methods for imaging MT dynamics in early zebrafish development, ranging from live imaging of tagged molecules to immunolabeling of fixed tissue11,12,13,14. 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 visualize this phenomenon. The method presented here leverages the power of 3-D imaging software to quantify the transition from dynamic to stable MT populations in a cross section of embryonic zebrafish tissue. In Protocol 2, the method is used to label a distinct population of nascent MTs and follow their nucleation and growth overtime.
MTs are notoriously difficult to image in their native state due to their propensity to depolymerize. Thus, the key component of this method is rapid fixation of MTs throughout the entire embryo. This is achieved by starting the fixation at physiological temperatures and using a buffer that both stabilizes the MTs and increases the permeability of the embryo. The fixation time is also important as curtailed fixation fails to arrest MTs while over-fixation can mask epitopes, interfering with antibody binding. The suggested fixation time of 3-4 h works with embryos that are in mid-gastrulation up to 24 h post-fertilization. Embryos towards the younger end of the time scale should be fixed for closer to 3 h while older embryos may need the entire 4 h. Even with proper fixation, the MTs will depolymerize with time so sectioning and immunolabeling must occur within one week of fixing.
Once the tissue is properly fixed, problems can arise with immunolabeling. The most common problem encountered has been poor penetration through the center of the tissue, particularly, if too many sections are incubated in the same well. Increasing the concentration of the primary antibody and incubation time for primary and secondary antibodies, combined with increasing the detergents to improve permeabilization of the embryos will ameliorate most of the immunolabeling problems. If the antibody labeling fails due to fixation issues or immunolabeling problems, it is possible to determine the cause by examining the antibody labeling pattern. Poor fixation will result in intense labeling in the membrane and diffuse labeling in the cytoplasm, while over-fixation will result in weak labeling that retains MT architecture. Poor penetration of the antibody, however, will appear as areas in the center of the tissue without labeling.
The ability to analyze MT images in a meaningful way is dependent on high quality imaging. To capture MT length in 3-D, the minimum Z-step size possible for the objective and numerical aperture should be used. Images shown here were captured with a 63X oil emersion objective with 1.4 numerical aperture producing the following: pixel = 240 nm, Z-step = 0.1 &#181;m, Z-stack size = 16.252 &#181;m. Because the width of a single MT is 25 nm, roughly 10 times below the limit of resolution for a light microscope, this metric cannot be accurately measured using this technique. Instead, only MT lengths equal to or greater than the minimum pixel size attainable in all three dimensions can be measured. Line and/or frame averaging can enhance the MT signal definition. MT analysis should be reserved for high quality sections. While tissue with poor fixation cannot be imaged and analyzed, mild overfixation can be counterbalanced by carefully increasing the laser intensity and gain to detect the weak signal while maintaining a good dynamic range. Poor antibody penetration, while not optimal, can be corrected by limiting image acquisition to well-labeled regions, resulting in imaging a thinner section (5-10 &#181;m). High background from labeling can be compensated for by adjusting the filter settings. However, if any of these adjustments are done, it is necessary to verify that the filters threshold acceptably on each plane of the Z-stack.
3-D image analysis software allows the experimenter to quantify MT length, area, angle, abundance, and other metrics in the 3-D space of fixed tissue sections. The method described here provides directions for obtaining such data using commercially available software. However, the filtering modules may be adapted to public domain software enhanced with relevant plugins and/or macros, making analysis available to all. Prior to analysis, raw images must be thresholded to avoid including background and non-specific signals in the quantification. Once analysis is completed and data are transferred to a workable spreadsheet, many inferences can be made from the data set. One of the calculations made here was Glu-tubulin streaks per &#946;-tubulin streaks, or the ratio of stable MTs to total MTs where 1 represents that the entire MT cytoskeleton was stabilized in an ROI. If the experimenter wishes to complement their quantitative data, generating a polished tagged image file format (TIFF) image with scale bars is effortless with 3-D image analysis software.
This assay allows the functional analysis of proteins implicated in MT assembly, in vivo. If immunolabeling is performed on alternating serial sections, this protocol could be used to study dynamic and stable MTs in the same embryo. In the future, modifications such as increased detergents or altered embedding angles will allow the use of these methods for older embryos and a wider range of anatomical questions.

Microtubules (MTs) are polymers of &#945;- and &#946;-tubulin that assemble into linear protofilaments, several of which combine to form a hollow tube1,2. 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 &#947;-tubulin ring complex (&#947;-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 MTs7,8. 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 ends11,12,13,14. 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 speed9,13,15. 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 &#945;-tubulin, such as acetylation and detyrosination, which accumulate on stable MTs over time16,17. 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 &#945;-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 &#945;-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 &#946;-tubulin) alongside markers for the centrosome (anti &#947;-tubulin) and nucleus (4&#39;,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 &#947;-tubulin to the centrosome is impaired, resulting in incomplete neural tube formation and neuronal defects24.

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

use of immunolabeling to analyze stable, dynamic, and nascent microtubules in the zebrafish embryo

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.

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 into the neural rod (11-12 somites), a stage of enhanced epithelialization, qualitatively fewer MTs are immunoreactive with the anti-Tyr-tubulin antibody (Figure 2E-H), especially in the ventral rod. In contrast, Glu-tubulin is scattered and punctate throughout the neural keel (Figure 3A-D), but is enriched in the ventral neural rod along MT tracts (Figure 3E-H). Arrowheads point to specific MT bundles or structures where labeling is increased.
Although both anti-Glu-tubulin and anti-Tyr-tubulin antibodies were produced in the same host species (preventing a double labeling experiment), these results indicate that stable and dynamic MT markers rarely overlap in the zebrafish hindbrain. Firstly, the ventral neural rod has more stable (Figure 3F) than dynamic (Figure 2F) MTs. The trend is reversed in the dorsal neural rod, consistent with a model of zebrafish neurulation in which the dorsal tissue remains dynamic until the neural tube is formed20. Secondly, while mitotic spindles are fully labeled with the Tyr-tubulin antibody in the neural keel (Figure 2D, arrowheads), only the base of the spindle, coincident with the centrosome, is labeled with the stability marker Glu-tubulin (Figure 3D, arrowheads). &#946;-tubulin immunofluorescence, common to both assays, informs the experimenter of the distribution of all MTs and provides a basis to dismiss non-specific labeling.
Measuring objects using 3-D image analysis software results in a large amount of data that can be organized into a convenient table (Table 2). To make length, count, and area measurements, we are using only a subset of the data that is available to analyze. One of the components of the data that we do not further analyze is the number of objects identified. This number is used as an internal quality control, as the number should not vary widely between like sections, and the ratio of nuclei to MTs should stay similar in a single treatment condition. An outlier is an indicator that either the analysis needs to be rerun with adjusted filters or that the image is too poorly labeled to analyze. Thus, all outlier images should be reanalyzed with adjusted settings. The outlier section should be examined for signs of poor labeling or physical damage that might result in unusual object counts. Once the analysis is finished and quality controlled, useful information can be recovered from the raw data such as average length of total MTs and stable MTs or the ratio of stable MTs to total MTs (Table 3). In addition to these measurements, many other metrics can be obtained using the 3-D image analysis software that can be used to draw inferences about MTs or their relation to other cellular structures (nucleus, centrosome, etc.).
De novo MT assembly assay 
The nocodazole treatment depolymerizes MTs resulting in diffuse labeling (Figure 4A, 4D, and 4G). As the MTs regrow, they extend from the centrosome (Figure 4B, 4E, and 4H), however, this may not be obvious in a single plane due to their non-planar trajectories (Figure 4C, 4F, and 4I). Nevertheless, some image analysis software are capable of measuring lengths in 3-D, enabling an assessment of MT growth after the nocodazole washout (Table 4). An important observation that can be obtained from the dataset in Table 4 is that the mean length of MTs appears to increase over time after the nocodazole washout in all regions of the neural tube analyzed. As mentioned above, other types of metrics obtained from 3-D image analysis software can provide cellular context to interpret the MT data (for example, ratio of MTs per nucleus).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/55792/55792fig1.jpg" /> 
Figure 1: Illustration of washout apparatus for de novo MT assembly assay. The inset is a close-up of the flow-through device made from mesh glued into a 50-mL centrifuge tube cut lengthwise. The mesh compartmentalizes the flow-through device such that multiple experimental groups can be processed simultaneously. During use, embryo medium is added to the syringe and slowly flows through the tubing to fill the flow-through device, providing a constant rinse to all experimental groups. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/55792/55792fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/55792/55792fig2.jpg" /> 
Figure 2: Use of immunolabeling to image dynamic MTs. Dechorionated embryos were fixed at appropriate stages (4-5 in A-D and 12-13 somites in E-H), transversely sectioned through the hindbrain, and immunolabeled with antibodies against &#946;-tubulin (green in A and E) to mark all MTs and tyrosinated &#945;-tubulin (red in B and F) to reveal dynamic MT populations. Highly dynamic MTs can be seen in the merged images (C, G) and their higher magnifications (D, H) as areas where yellow label is visible (arrowheads in D, H). Scale bars = 25 &#181;m (A-C and E-G) and 10 &#181;m (D and H). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/55792/55792fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/55792/55792fig3.jpg" /> 
Figure 3: Use of immunolabeling to image stable MTs. Dechorionated embryos were fixed, sectioned through the hindbrain, and immunolabeled at appropriate stages (4-5 somites in A-D and 12-13 somites in E-H). Stable MTs are labeled with antibodies against the detyrosinated form of &#945;-tubulin (Glu-tubulin) (red in B and F) while total MTs were visualized with a general &#946;-tubulin antibody (green in A and E). Red and yellow signals in merged images (C, G) and their higher magnifications (D, H) represent areas of high MT stability (arrowheads in D, H). Scale bars = 25 &#181;m (A-C and E-G) and 10 &#181;m (D and H). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/55792/55792fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/55792/55792fig4.jpg" /> 
Figure 4: Use of immunolabeling to image nascent MTs. Dechorionated embryos were fixed at 4-5 somites and transversely sectioned through the hindbrain. Sections were immunolabeled with &#946;-tubulin (D, E, and F) to mark growing MTs and &#947;-tubulin (A, B, and C) to mark the nucleation point/centrosome. A dorsal region of the neural tube is boxed in (A, D; B, E and C-F) and shown at higher magnification (G, H, I, respectively) to reveal nuclei (DAPI, blue), centrioles (&#947;-tubulin, red) and total MTs (&#946;-tubulin, green). White arrowheads: colocalization of MTs and centrioles; yellow arrowheads: the second centriole of a cell is visible. Scale bars = 25 &#181;m (A-F) and 10 &#181;m (G-I). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/55792/55792fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Table 1" src="/files/ftp_upload/55792/55792table1.jpg" /> 
Table 1: Default settings for filtering objects in 3-D image analysis software. 
<img alt="Table 2" src="/files/ftp_upload/55792/55792table2.jpg" /> 
Table 2: Representative raw data set obtained using 3-D image analysis software to analyze stable MTs. Each column represents measurements from a single section. Min: smallest measurement; Max: largest measurement; SD: standard deviation; SE: standard error.
<img alt="Table 3" src="/files/ftp_upload/55792/55792table3.jpg" /> 
Table 3: Examples of datasets that can be obtained from 3-D image analysis software to quantify stable MTs. Select measurements of the mean length of total (&#946;-tubulin) and stable (Glu-tubulin) MTs calculated by taking the average of the mean skeletal length for the relevant label from all samples (refer to Table 2) and the ratio of stable to total MTs (Glu-tubulin streaks per &#946;-tubulin streaks) calculated by taking the average &#946;-tubulin count divided by the average Glu-tubulin count.
<img alt="Table 4" src="/files/ftp_upload/55792/55792table4.jpg" /> 
Table 4: Examples of datasets that can be obtained from 3-D image analysis software to analyze de novo MT assembly. Representative results from the de novo MT assembly experiment, comparing datasets obtained for three recovery time points (1, 5 and 10 min) after nocodazole washout. For each time point, measurements obtained for nuclear count, centrioles (&#947;-tubulin puncta), number of total MTs (&#946;-tubulin streaks), are shown for selected regions of the imaged analyzed (cross section of the developing neural tube).

Watch this Scientific Journal Video about Use of Immunolabeling to Analyze Stable, Dynamic, and Nascent Microtubules in the Zebrafish Embryo at JoVE.com

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

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.

Microtubules (MTs) are dynamic and fragile structures that are challenging to image in vivo, particularly in vertebrate embryos. Immunolabeling methods ...

use-immunolabeling-to-analyze-stable-dynamic-nascent-microtubules

Nanyang Technological University

Research

JoVE Journal

Developmental Biology

8.2K Views.  University of Maryland, Baltimore County. Immunolabeling methoden voor het analyseren van verschillende populaties van microtubuli in de ontwikkelende hersenen van de zebravis zijn hier beschreven, die over het algemeen van toepassing zijn op andere weefsels. Het eerste protocol schetst een geoptimaliseerde methode voor immunolabeling stabiele en dynamische microtubuli. Het tweede protocol biedt een methode om beeld en kwantificeren van ontluikende microtubuli specifiek.

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

Labeling and Imaging Cells in the Zebrafish Hindbrain

Key to understanding the morphogenetic processes that shape the early vertebrate embryo is the ability to image cells at high resolution. In zebrafish embryos, injection of plasmid DNA results in mosaic expression, allowing for the visualization of single cells or small clusters of cells 1 . We describe how injection of plasmid DNA encoding membrane-targeted Green Fluorescent Protein (mGFP) under the control of a ubiquitous promoter can be used for imaging cells undergoing neurulation. Central to this protocol is the methodology for imaging labeled cells at high resolution in sections and also in real time. This protocol entails the injection of mGFP DNA into young zebrafish embryos. Embryos are then processed for vibratome sectioning, antibody labeling and imaging with a confocal microscope. Alternatively, live embryos expressing mGFP can be imaged using time-lapse confocal microscopy. We have previously used this straightforward approach to analyze the cellular behaviors that drive neural tube formation in the hindbrain region of zebrafish embryos 2. The fixed preparations allowed for unprecedented visualization of cell shapes and organization in the neural tube while live imaging complemented this approach enabling a better understanding of the cellular dynamics that take place during neurulation.

Key to understanding the morphogenetic processes that shape the early embryo is the ability to image cells at high resolution. We describe here a technique for labeling single cells or small clusters of cells in whole zebrafish embryos with membrane-targeted Green Fluorescent Protein.

Key to understanding the morphogenetic processes that shape the early vertebrate embryo is the ability to image cells at high resolution. In zebrafish ...

Neuroscience

Analyzing In Vivo Cell Migration using Cell Transplantations and Time-lapse Imaging in Zebrafish Embryos

Cell migration is key to many physiological and pathological conditions, including cancer metastasis. The cellular and molecular bases of cell migration have been thoroughly analyzed in vitro. However, in vivo cell migration somehow differs from in vitro migration, and has proven more difficult to analyze, being less accessible to direct observation and manipulation. This protocol uses the migration of the prospective prechordal plate in the early zebrafish embryo as a model system to study the function of candidate genes in cell migration. Prechordal plate progenitors form a group of cells which, during gastrulation, undergoes a directed migration from the embryonic organizer to the animal pole of the embryo. The proposed protocol uses cell transplantation to create mosaic embryos. This offers the combined advantages of labeling isolated cells, which is key to good imaging, and of limiting gain/loss of function effects to the observed cells, hence ensuring cell-autonomous effects. We describe here how we assessed the function of the TORC2 component Sin1 in cell migration, but the protocol can be used to analyze the function of any candidate gene in controlling cell migration in vivo.

Analyzing In Vivo Cell Migration using Cell Transplantations and Time-lapse Imaging in Zebrafish Embryos

Combining cell transplantation, cytoskeletal labeling and loss/gain of function approaches, this protocol describes how the migrating zebrafish prospective prechordal plate can be used to analyze the function of a candidate gene in in vivo cell migration.

Cell migration is key to many physiological and pathological conditions, including cancer metastasis. The cellular and molecular bases of cell migration ...

Observing Mitotic Division and Dynamics in a Live Zebrafish Embryo

Mitosis is critical for organismal growth and differentiation. The process is highly dynamic and requires ordered events to accomplish proper chromatin condensation, microtubule-kinetochore attachment, chromosome segregation, and cytokinesis in a small time frame. Errors in the delicate process can result in human disease, including birth defects and cancer. Traditional approaches investigating human mitotic disease states often rely on cell culture systems, which lack the natural physiology and developmental/tissue-specific context advantageous when studying human disease. This protocol overcomes many obstacles by providing a way to visualize, with high resolution, chromosome dynamics in a vertebrate system, the zebrafish. This protocol will detail an approach that can be used to obtain dynamic images of dividing cells, which include: in vitro transcription, zebrafish breeding/collecting, embryo embedding, and time-lapse imaging. Optimization and modifications of this protocol are also explored. Using H2A.F/Z-EGFP (labels chromatin) and mCherry-CAAX (labels cell membrane) mRNA-injected embryos, mitosis in AB wild-type, auroraBhi1045, and esco2hi2865 mutant zebrafish is visualized. High resolution live imaging in zebrafish allows one to observe multiple mitoses to statistically quantify mitotic defects and timing of mitotic progression. In addition, observation of qualitative aspects that define improper mitotic processes (i.e., congression defects, missegregation of chromosomes, etc.) and improper chromosomal outcomes (i.e., aneuploidy, polyploidy, micronuclei, etc.) are observed. This assay can be applied to the observation of tissue differentiation/development and is amenable to the use of mutant zebrafish and pharmacological agents. Visualization of how defects in mitosis lead to cancer and developmental disorders will greatly enhance understanding of the pathogenesis of disease.

Mitosis is critical to every living organism and defects often lead to cancer and developmental disorders. Using this imaging protocol and zebrafish as a model system, researchers can visualize mitosis in a live vertebrate organism and the multitude of defects that arise when mitotic processes are defective.

Mitosis is critical for organismal growth and differentiation. The process is highly dynamic and requires ordered events to accomplish proper chromatin ...

Visualizing Multiciliated Cells in the Zebrafish Through a Combined Protocol of Whole Mount Fluorescent In Situ Hybridization and Immunofluorescence

In recent years, the zebrafish embryo has emerged as a popular model to study developmental biology due to traits such as ex utero embryo development and optical transparency. In particular, the zebrafish embryo has become an important organism to study vertebrate kidney organogenesis as well as multiciliated cell (MCC) development. To visualize MCCs in the embryonic zebrafish kidney, we have developed a combined protocol of whole-mount fluorescent in situ hybridization (FISH) and whole mount immunofluorescence (IF) that enables high resolution imaging. This manuscript describes our technique for co-localizing RNA transcripts and protein as a tool to better understand the regulation of developmental programs through the expression of various lineage factors.

Visualizing Multiciliated Cells in the Zebrafish Through a Combined Protocol of Whole Mount Fluorescent In Situ Hybridization and Immunofluorescence

Cilia development is vital to proper organogenesis. This protocol describes an optimized method to label and visualize ciliated cells of the zebrafish.

In recent years, the zebrafish embryo has emerged as a popular model to study developmental biology due to traits such as ex utero embryo development and ...

Fluorescent Protein Tagging in Zebrafish Larvae Using CRISPR/Cas9 Knock-In

Fluorescence Labeling to Visualize Low-Expressed Proteins in Zebrafish

CRISPR/Cas9-mediated knock-in (KI) technology allows for easier fluorescent-protein tagging in zebrafish (Danio rerio), a preferred model organism for in vivo imaging due to its transparency during the early developmental stage. Here, we provide a detailed protocol for performing high-efficiency fluorescence gene KI, rapid screening for KI founders, and low-abundance protein tracing in zebrafish larvae, which will lay a critical foundation for subsequent physio-pathological studies in zebrafish. The current protocol includes complete steps for the sgRNA design for the gene of interest, sgRNA in vitro transcription, Cas9 mRNA in vitro transcription, in vivo sgRNA screen for the one with the highest efficiency, donor plasmid design and construction, microinjection in zebrafish larvae, KI founder screen and zebrafish live imaging. Critical steps, troubleshooting tips, quality control methods, and advantages and applications of this protocol are included and discussed. This protocol assures quick and accurate results at a low cost and has been validated by multiple trials.

Here, we present a protocol to label proteins with a fluorescence protein tag in zebrafish larvae, a newly developed and modified in vivo system especially useful for visualizing low-abundance proteins in zebrafish.

CRISPR/Cas9-mediated knock-in (KI) technology allows for easier fluorescent-protein tagging in zebrafish (Danio rerio), a preferred model organism for in ...

Genetics

Whole Mount Immunohistochemistry in Zebrafish Embryos and Larvae

Immunohistochemistry is a widely used technique to explore protein expression and localization during both normal developmental and disease states. Although many immunohistochemistry protocols have been optimized for mammalian tissue and tissue sections, these protocols often require modification and optimization for non-mammalian model organisms. Zebrafish are increasingly used as a model system in basic, biomedical, and translational research to investigate the molecular, genetic, and cell biological mechanisms of developmental processes. Zebrafish offer many advantages as a model system but also require modified techniques for optimal protein detection. Here, we provide our protocol for whole-mount fluorescence immunohistochemistry in zebrafish embryos and larvae. This protocol additionally describes several different mounting strategies that can be employed and an overview of the advantages and disadvantages each strategy provides. We also describe modifications to this protocol to allow detection of chromogenic substrates in whole mount tissue and fluorescence detection in sectioned larval tissue. This protocol is broadly applicable to the study of many developmental stages and embryonic structures.

Here, we present a protocol for fluorescent antibody-mediated detection of proteins in whole preparations of zebrafish embryos and larvae.

Immunohistochemistry is a widely used technique to explore protein expression and localization during both normal developmental and disease states. ...

Antibody Uptake Assay for Tracking Notch/Delta Endocytosis During the Asymmetric Division of Zebrafish Radial Glia Progenitors

Asymmetric cell division (ACD), which produces two daughter cells of different fates, is fundamental for generating cellular diversity. In the developing organs of both invertebrates and vertebrates, asymmetrically dividing progenitors generates a Notchhi self-renewing and a Notchlo differentiating daughter. In the embryonic zebrafish brain, radial glia progenitors (RGPs)-the principal vertebrate neural stem cells-mostly undergo ACD to give birth to one RGP and one differentiating neuron. The optical clarity and easy accessibility of zebrafish embryos make them ideal for in vivo time-lapse imaging to directly visualize how and when the asymmetry of Notch signaling is established during ACD. Recent studies have shown that dynamic endocytosis of the Notch ligand DeltaD plays a crucial role in cell fate determination during ACD, and the process is regulated by the evolutionarily conserved polarity regulator Par-3 (also known as Pard3) and the dynein motor complex. To visualize the in vivo trafficking patterns of Notch signaling endosomes in mitotic RGPs, we have developed this antibody uptake assay. Using the assay, we have uncovered the dynamicity of DeltaD-containing endosomes during RGP division.

This work develops an antibody uptake assay for imaging intra-lineage Notch/DeltaD signaling in dividing radial glia progenitors of the embryonic zebrafish brain.

Asymmetric cell division (ACD), which produces two daughter cells of different fates, is fundamental for generating cellular diversity. In the developing ...

Imaging Glycans in Zebrafish Embryos by Metabolic Labeling and Bioorthogonal Click Chemistry

Imaging glycans in vivo has recently been enabled using a bioorthogonal chemical reporter strategy by treating cells or organisms with azide- or alkyne-tagged monosaccharides1, 2. The modified monosaccharides, processed by the glycan biosynthetic machinery, are incorporated into cell surface glycoconjugates. The bioorthogonal azide or alkyne tags then allow covalent conjugation with fluorescent probes for visualization, or with affinity probes for enrichment and glycoproteomic analysis. This protocol describes the procedures typically used for noninvasive imaging of fucosylated glycans in zebrafish embryos, including: 1) microinjection of one-cell stage embryos with GDP-5-alkynylfucose (GDP-FucAl), 2) labeling fucosylated glycans in the enveloping layer of zebrafish embryos with azide-conjugated fluorophores via biocompatible Cu(I)-catalyzed azide-alkyne cycloaddition (CuAAC), and 3) imaging by confocal microscopy3. The method described here can be readily extended to visualize other classes of glycans, e.g. glycans containing sialic acid4 and N-acetylgalactosamine5, 6, in developing zebrafish and in other living organisms.

A click-chemistry based method that allows for the rapid, noninvasive, and robust labeling of alkyne-tagged glycans in zebrafish embryos is described. Fucosylated glycans in the enveloping layer of zebrafish embryos in the late gastrulation stage were imaged in this study.

Imaging glycans in vivo has recently been enabled using a bioorthogonal chemical reporter strategy by treating cells or organisms with azide- or ...

Biology

Flat Mount Preparation for Observation and Analysis of Zebrafish Embryo Specimens Stained by Whole Mount In situ Hybridization

The zebrafish embryo is now commonly used for basic and biomedical research to investigate the genetic control of developmental processes and to model congenital abnormalities. During the first day of life, the zebrafish embryo progresses through many developmental stages including fertilization, cleavage, gastrulation, segmentation, and the organogenesis of structures such as the kidney, heart, and central nervous system. The anatomy of a young zebrafish embryo presents several challenges for the visualization and analysis of the tissues involved in many of these events because the embryo develops in association with a round yolk mass. Thus, for accurate analysis and imaging of experimental phenotypes in fixed embryonic specimens between the tailbud and 20 somite stage (10 and 19 hours post fertilization (hpf), respectively), such as those stained using whole mount in situ hybridization (WISH), it is often desirable to remove the embryo from the yolk ball and to position it flat on a glass slide. However, performing a flat mount procedure can be tedious. Therefore, successful and efficient flat mount preparation is greatly facilitated through the visual demonstration of the dissection technique, and also helped by using reagents that assist in optimal tissue handling. Here, we provide our WISH protocol for one or two-color detection of gene expression in the zebrafish embryo, and demonstrate how the flat mounting procedure can be performed on this example of a stained fixed specimen. This flat mounting protocol is broadly applicable to the study of many embryonic structures that emerge during early zebrafish development, and can be implemented in conjunction with other staining methods performed on fixed embryo samples.

Flat Mount Preparation for Observation and Analysis of Zebrafish Embryo Specimens Stained by Whole Mount In situ Hybridization

The zebrafish embryo is an excellent model for developmental biology research. During embryogenesis, zebrafish develop with a yolk mass, which presents three-dimensional challenges for sample observation and analysis. This protocol describes how to create two-dimensional flat mount preparations of whole mount in situ (WISH) stained zebrafish embryo specimens.

The zebrafish embryo is now commonly used for basic and biomedical research to investigate the genetic control of developmental processes and to model ...

Elucidating Microglia Behavior in Zebrafish Optic Tectum Development

Live Imaging and Characterization of Microglia Dynamics in the Zebrafish Embryo

Microglia are highly dynamic cells and their migration and colonization of the brain parenchyma is a crucial step for proper brain development and function. Externally developing zebrafish embryos possess optical transparency, which along with well-characterized transgenic reporter lines that fluorescently label microglia, make zebrafish an ideal vertebrate model for such studies. In this paper, we take advantage of the unique features of the zebrafish model to visualize the dynamics of microglia cells in vivo and under physiological conditions. We use confocal microscopy to record a timelapse of microglia cells in the optic tectum of the zebrafish embryo and then, extract tracking data using the IMARIS 10.0 software to obtain the cells' migration path, mean speed, and distribution in the optic tectum at different developmental stages. This protocol can be a useful tool to elucidate the physiological significance of microglia behavior in various contexts, contributing to a deeper characterization of these highly motile cells.

Author Spotlight: Using Zebrafish to Explore Microglia Migration During Brain Development

We demonstrate a method that takes advantage of fast scanning confocal microscopy to perform live imaging of microglia cells in the developing zebrafish optic tectum, allowing for the analysis of the dynamics of these cells in vivo.

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

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