The authors thank Dr. Dick Campbell (UC Irvine) for discussions about the original protocol for generating and maintaining nerve-free animals, Ms. Rui Wang for help with adapting the syringe and needle technique, and Ms. Danielle Hagstrom and Dr. Rob Steele (UC Irvine) for comments on the manuscript. This work was supported by the RCSA and NSF grant CMMI-1463572.

1. Double Colchicine Treatment
<ol>
	<li>Make a 0.4% colchicine (weight/volume) solution in Hydra medium3,4,17. 
	Caution: Colchicine is acutely toxic, fatal if swallowed, may cause genetic defects, and may cause eye damage. Handle the powder in a fume hood and wear full Personal Protective Equipment (PPE).</li>
	<li>Incubate Hydra vulgaris (AEP strain was used here) that have been starved for 24 h in 0.4% colchicine at a ratio of 5 Hydra per mL of colchicine solution in a Petri dish for 8 h at room temperature in the dark. 
	Note: 5 Hydra/mL colchicine is a guideline for determining how much solution to use to avoid overcrowding the dish with Hydra. Use the same volume of solution for subsequent cleanings and solution changes.</li>
	<li>Remove the colchicine solution and replace with clean Hydra medium without colchicine. Wash the Hydra 5 times by serial transfer with a glass Pasteur pipette into clean Hydra medium before transferring to 50 &#181;g/mL rifampicin in Hydra medium. Keep the Hydra in an 18 &#176;C incubator. 
	Note: Sufficient 1,000X rifampicin stock (50 mg/mL) in dimethyl sulfoxide (DMSO) for 1-2 weeks of treatment can be stored at 4 &#176;C. The exact amount can be determined by the total volume of solution used each day. For example, if there are 2 dishes, each containing 10 mL of solution that needs to be changed twice daily, a total of 40 mL of solution will be used in one day, corresponding to 40 &#181;L of 1,000X stock per day or 560 &#181;L over a two week period. The stock is then diluted 1:1000 in Hydra medium upon use. 
	Caution: DMSO is a combustible liquid and readily penetrates skin, allowing other dissolved chemicals into the body. Handle the solvent in a fume hood and wear full PPE. Of note, DMSO freezes at 4 &#176;C</li>
	<li>Change the rifampicin-containing Hydra medium twice daily until the Hydra stop expelling cells into the medium, which is generally by 1 week post-treatment. At this point, the medium can be changed once daily. During the days following the treatment, the Hydra will completely lose their tentacles. Avoid having the Hydra in contact with one another, as they may fuse together and result in oddly shaped Hydra (Figure 2A).
	<ol>
		<li>To prevent contact, avoid swirling the dish in a circular motion. Instead, gently agitate the dish in vertical and horizontal directions until the Hydra are spread apart. Inspect the dish upon placing the Hydra into the 18 &#176;C incubator and adjust as necessary. 
		Note: For the days that the medium is changed twice, change the medium once in the morning and again in the afternoon/evening.</li>
	</ol>
	</li>
	<li>Once the tentacles begin to form, begin force-feeding and burping the Hydra 3 to 4 times a week (see Sections 2 and 3). About 8-9 days following colchicine treatment, the Hydra will begin to grow their tentacles back. 
	Note: Tentacle regrowth varies among individuals. Some may take longer than 8 - 9 days before showing signs of tentacle growth. Those that do not regrow their tentacles as well as oddly shaped (Figure 2B) animals or animals too small to be fed should be removed. These Hydra will likely not survive the second treatment. The Hydra may also bud. However, some of the buds may still have interstitial cells and be able to eat on their own.
	<ol>
		<li>Remove any buds that can eat without assistance and detach from the parent animal. Identify these animals by adding live Artemia to the feeding dish and observing whether or not the animals catch and eat the Artemia on their own. 1 or 2 Hydra may also be able to eat on their own. These should also be discarded. 
		Note: Nerve-free Hydra have a characteristic balloon-like morphology, and tentacles that are shorter and thinner than normal (due to loss of nematocytes) and can thus easily be distinguished from normal looking animals (Figure 1A, 1B).</li>
	</ol>
	</li>
	<li>Three weeks following the first colchicine treatment, repeat the colchicine treatment (steps 1.1 - 1.5). A second colchicine treatment is necessary to eliminate the remaining interstitial cells and nerve cells3.</li>
</ol>
2. Force-Feeding
<ol>
	<li>Add Artemia cysts to a narrow and tall glass container that tapers at the bottom. Fill the container with Artemia water (6.72 M NaCl). Avoid exceeding 1 g of cysts per 1 L of water for a higher hatch yield.
	<ol>
		<li>Cover the top of the container with parafilm and insert a 10 mL serological pipette through the parafilm into the container. Provide aeration by attaching tubing to an aquarium air pump and fitting the tubing around the pipette. Make sure that the pipette tip reaches the bottom of the container and that no cysts are settled at the bottom. The Artemia will hatch after 48 h. 
		Note: There are many different ways to hatch Artemia that may work just as well.</li>
	</ol>
	</li>
	<li>Strain the Artemia from the Artemia water in an Artemia net (available from aquarium supply companies) and wash them for about 20 s in DI water before placing them in a dish with Hydra medium. The salinity of Artemia water is too high for Hydra, so the Artemia must be washed before they are used.</li>
	<li>Under a dissecting microscope, euthanize the Artemia by lightly squeezing them with a pair of fine forceps. Avoid squeezing hard enough to expel the guts, as this will stick to the forceps and make feeding difficult. Lightly squeezing the Artemia before feeding it to the Hydra will help with the digestion process14. Place the freshly killed Artemia close to the Hydra in the dish to facilitate fast feeding. 
	Note: All subsequent steps are done under a dissecting microscope.</li>
	<li>Use one pair of forceps to hold the Hydra by the peduncle. Continue holding the peduncle during the process of feeding the Hydra. Using a second pair of forceps, pinch the body column in order to make the Hydra contract.</li>
	<li>While holding the tips of the second pair of forceps together, tap at the center of the hypostome (the domed structure at the oral end of the animal). This sometimes causes the mouth to open. If the mouth does not open by tapping, puncture the mouth by inserting the forceps into the center of the hypostome and then slightly release the pressure on the tips of the forceps. This should stretch out the mouth opening made by the puncture. 
	Note: The Hydra may deflate and collapse when the mouth is opened (Figure 2C). If this occurs, the Artemia may still be inserted into the Hydra. If it is too difficult to do so, move on to the next Hydra and return to the original Hydra some time later and try again. The Hydra tend not to deflate as much during subsequent mouth openings.</li>
	<li>Quickly pick up Artemia with the forceps and insert them into the Hydra&#39;s gastric cavity. Insert as many Artemia as possible until the gastric cavity is full and more Artemia cannot be inserted without damaging the Hydra, accidentally pulling out any Artemia inside, or preventing the mouth from closing. On average, this is 5 - 6 Artemia, however up to 12 have been fed to the larger animals.
	<ol>
		<li>If the mouth begins to close, stretch open again with the forceps as described above; however, caution should be taken as any Artemia already inside the animal may begin to come out when the mouth is reopened.</li>
		<li>If the Hydra is too small for a whole Artemia, cut the Artemia using a scalpel and feed the Hydra smaller pieces. If the Artemia does not stay inside the Hydra, it may be necessary to press the forceps against the Artemia to keep it inside the Hydra until its mouth closes.</li>
	</ol>
	</li>
	<li>Transfer fed Hydra with a glass Pasteur pipette, carefully to avoid accidental burping, to a dish with fresh 50 &#181;g/mL rifampicin in Hydra medium. If an Artemia was expelled from the Hydra while transferring, reinsert it while in the new dish. 
	Note: A glass pipette is used to transfer the Hydra, as it has been found that Hydra stick less to glass compared to plastic. The length of the pipette does not matter, but using 5 inch pipettes may be somewhat easier.</li>
</ol>
3. Burping
<ol>
	<li>Burp the Hydra to remove undigested material any time between 8 and 20 h after feeding.</li>
	<li>Sand down the point of a 30G hypodermic needle with P320 or similar grit sandpaper until the tip is flat. 
	Note: A 27G hypodermic needle would also work, but the smaller tip of the higher gauge is preferable.</li>
	<li>Attach the needle to a disposable 1 mL plastic syringe and fill the syringe with fresh 50 &#181;g/mL rifampicin in Hydra medium. 
	Note: Burping a single Hydra takes about 0.05 mL to 0.1 mL of solution. A 1 mL syringe is preferable since controlling the force and volume of the solution coming out is more difficult with a larger volume syringe.</li>
	<li>Under a dissecting microscope, hold the peduncle of the Hydra with fine point forceps and tap at the center of the hypostome with the needle. If the mouth does not open, insert forceps into the hypostome and open the mouth as described above for feeding. 
	Note: All subsequent steps are done under a dissecting microscope.</li>
	<li>Use the syringe to flush, very gently to avoid blowing away the entire animal, the gastric cavity with the 50 &#181;g/mL rifampicin solution until all debris has been expelled. The needle does not necessarily need to be inserted into the Hydra if the size of the Hydra does not permit. The needle may be held close to the mouth opening and pointed directly towards the mouth.</li>
	<li>Using a glass Pasteur pipette, transfer burped Hydra to a dish with fresh 50 &#181;g/mL rifampicin in Hydra medium.</li>
</ol>
4. Quality Control Via Immunohistochemistry
NOTE: The following protocol is adapted from protocols by Shenk, M. A, et al.18, and B&#246;ttger, A19. All steps are done at room temperature (RT) unless otherwise noted. A nutator can be used for the incubation steps and may improve staining quality. However, if the Hydra get tangled up with one another, all steps can also be performed without.
<ol>
	<li>Prepare the blocking solution: 10% fetal bovine serum (FBS) and 1% DMSO in 1x phosphate-buffered saline (PBS). Store this solution at 4 &#176;C until use (steps 4.6 and 4.11). The solution can be stored for 1 - 2 days. 
	Note: All solutions used in this protocol must be properly collected as hazardous waste.</li>
	<li>Relax Hydra in 200 &#181;L of 2% urethane in Hydra medium for 1 min in 1.7 mL microcentrifuge tubes. Use 5 Hydra per tube for each of the 4 conditions: nerve-free, untreated, untreated with no primary antibody, and untreated with no secondary antibody. 
	Note: Do not exceed 1 min. The timing here is critical as animals will be in bad shape after spending too much time in urethane.</li>
	<li>Remove the urethane and fix the Hydra in 200 &#181;L of 4% paraformaldehyde (PFA) in Hydra medium for 15 min.</li>
	<li>Wash the samples 3 times with 1x PBS for 10 min each. 
	Note: All washes with PBS and PBSTx are done with 500 &#181;L of solution.</li>
	<li>Permeabilize with 500 &#181;L of 0.5% Triton X-100 in PBS for 15 min.</li>
	<li>Remove the 0.5% Triton X-100 and add 500 &#181;L of the blocking solution. Block the samples for at least 1 h.</li>
	<li>Dilute the anti-tyrosine-tubulin antibody 1:200 in blocking solution. 
	Note: This concentration was determined experimentally. If the signal in the controls is found to be too weak, the concentration may need to be increased. If there is nonspecific binding, the concentration may need to be decreased. Pre-incubation of the antibody may also help reduce nonspecific binding.</li>
	<li>Remove the blocking solution from the samples and add 200 &#181;L of the primary antibody to the nerve-free Hydra, untreated controls, and untreated controls with no secondary. For the untreated controls with no primary, only add 200 &#181;L of blocking solution without the antibody.</li>
	<li>Incubate the samples overnight (&#62;12 h) at 4 &#176;C. 
	Note: Alternatively, incubate 5 - 6 h at RT.</li>
	<li>Remove the primary antibody and wash the samples extensively with 0.3% Triton X-100 in 1x PBS (PBSTx). 
	Note: Save the primary antibody and store at 4 &#176;C, as it can be reused at least 2 - 3 times.</li>
	<li>Dilute goat anti-mouse hP secondary antibody 1:500 in blocking solution. Add 200 &#181;L to the nerve-free Hydra, untreated controls, and untreated controls with no primary. For the untreated controls with no secondary, only add 200 &#181;L of blocking solution without the antibody. 
	Note: Alternatively, a fluorescent secondary antibody can be used, for which steps 4.13 - 4.17 are not needed. Using a fluorescent secondary saves time and is generally adequate, but the hP secondary provides increased sensitivity. The concentration of secondary was determined experimentally. If the signals in the controls are found to be too weak, the concentration may need to be increased. If there is nonspecific binding, the concentration may need to be decreased.</li>
	<li>Incubate the samples overnight at 4 &#176;C.</li>
	<li>Remove the secondary antibody and wash the samples extensively with PBSTx.</li>
	<li>Prepare 1x PBT: 0.2% bovine serum albumin (weight/volume), and 0.05% Tween20 in 1x PBS. Incubate the samples in 1x PBT for 30 min.</li>
	<li>Remove the 1x PBT and incubate the samples in 1:1,000 NHS-fluorescein and 1:10,000 H2O2 in 1x PBT for 15 min in the dark. From this step on, keep the samples in the dark as much as possible, as the fluorescent signal will decrease as they are exposed to light. 
	Note: NHS-fluorescein was prepared following a detailed FISH protocol by King, R. S. and Newmark, P. A.20</li>
	<li>Wash the samples 3 times with PBSTx quickly, then 2 times for 30 min.</li>
	<li>Leave the samples in PBSTx overnight at 4 &#176;C to continue washing.</li>
	<li>Do a few more washes with 1x PBSTx. To visualize cell nuclei, carry out the following optional steps for DNA counterstaining using 4&#39;, 6-diamindino-2-phenylindole, dihydrochloride (DAPI). Otherwise, the samples may be imaged now.</li>
	<li>Dilute 5 mg/mL DAPI stock to a working concentration of 1:500 in PBSTx and add 200 &#181;L to each tube. Incubate the samples for 30 min. 
	Caution: DAPI is a known carcinogen. Wear full PPE.</li>
	<li>Remove the DAPI and wash the samples 2 - 3 times with PBSTx before imaging with fluorescence microscopy.</li>
</ol>

<ol><li>Bode, H. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((The+interstitial+cell+lineage+of+Hydra%3A+a+stem+cell+system+that+arose+early+in+evolution%5BTitle%5D)+AND+%22J.+Cell.+Sci%22%5BJournal%5D)">The interstitial cell lineage of Hydra: a stem cell system that arose early in evolution.</a> J. Cell. Sci. 109, 1155-1164 (1996).</li>
<li>Hager, G., David, C. N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Pattern+of+differentiated+nerve+cells+in+hydra+is+determined+by+precursor+migration%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">Pattern of differentiated nerve cells in hydra is determined by precursor migration.</a> Development. 124, 569-576 (1997).</li>
<li>Campbell, R. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Elimination+of+Hydra+interstitial+and+nerve+cells+by+means+of+colchicine%5BTitle%5D)+AND+%22J.+Cell.+Sci%22%5BJournal%5D)">Elimination of Hydra interstitial and nerve cells by means of colchicine.</a> J. Cell. Sci. 21, 1-13 (1976).</li>
<li>Marcum, B. A., Campbell, R. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Development+of+Hydra+lacking+nerve+and+interstitial+cells%5BTitle%5D)+AND+%22J.+Cell.+Sci%22%5BJournal%5D)">Development of Hydra lacking nerve and interstitial cells.</a> J. Cell. Sci. 29, 17-33 (1978).</li>
<li>Burns, R. G. <a target="_blank" href="http://www.sciencedirect.com/science/article/pii/001448277390517X">3H-colchicine binding: Failure to detect any binding to soluble proteins from various lower organisms.</a> Exp. Cell. Res. 81, 285-292 (1973).</li>
<li>Lee, H. -T., Campbell, R. D. <a target="_blank" href="https://www.jstor.org/stable/1541055?seq=1#page_scan_tab_contents">Development and Behavior of an Intergeneric Chimera of Hydra (Pelmatohydra oligactis Interstitial Cells Hydra attenuata Epithelial Cells).</a> Biol. Bull. 157 (2), 288-296 (1979).</li>
<li>Novak, P. Preparing Hydra viridis with Nerve Cells and No Interstitial Cells, or with Neither of These Cell Types. <a target="_blank" href="http://scholar.google.com/scholar?hl=en&safe=off&q=author%3aNovak%2C+P+%22Hydra%3A+Research+Methods%22">Hydra: Research Methods</a>. , Plenum Press. New York. 295-297 (1983).</li>
<li>Wanek, N., Marcum, B. A., Lee, H. -T., Chow, M., Campbell, R. D. <a target="_blank" href="https://www.researchgate.net/publication/230091645_Effect_of_hydrostatic_pressure_on_morphogenesis_in_nerve-free_hydra">Effect of hydrostatic pressure on morphogenesis in nerve-free Hydra.</a> J. Exp. Zool. 211, 275-280 (1980).</li>
<li>Minobe, S., Koizumi, O., Sugiyama, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Nerve+cell+differentiation+in+nerve-free+tissue+of+epithelial+Hydra+from+precursor+cells+introduced+by+grafting%5BTitle%5D)+AND+%22Dev.+Biol%22%5BJournal%5D)">Nerve cell differentiation in nerve-free tissue of epithelial Hydra from precursor cells introduced by grafting.</a> Dev. Biol. 172 (1), 170-181 (1995).</li>
<li>Miljkovic-Licina, M., Chera, S., Ghila, L., Galliot, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Head+regeneration+in+wild-type+hydra+requires+de+novo+neurogenesis%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">Head regeneration in wild-type hydra requires de novo neurogenesis.</a> Development. 134 (6), 1191-1201 (2007).</li>
<li>Wenger, Y., Buzgariu, W., Galliot, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Loss+of+neurogenesis+in+Hydra+leads+to+compensatory+regulation+of+neurogenic+and+neurotransmission+genes+in+epithelial+cells%5BTitle%5D)+AND+%22Phil.+Trans.+R.+Soc.+B%22%5BJournal%5D)">Loss of neurogenesis in Hydra leads to compensatory regulation of neurogenic and neurotransmission genes in epithelial cells.</a> Phil. Trans. R. Soc. B. 371 (20150040), (2015).</li>
<li>Campbell, R. D., Josephson, R. K., Schwab, W. E., Rushforth, N. B. <a target="_blank" href="https://www.ncbi.nlm.nih.gov/pubmed/958390">Excitability of nerve-free Hydra.</a> Nature. 262, 388-390 (1976).</li>
<li>Takaku, Y., Hwang, J. S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Innexin+gap+junctions+in+nerve+cells+coordinate+spontaneous+contractile+behavior+in+Hydra+polyps%5BTitle%5D)+AND+%22Sci.+Rep%22%5BJournal%5D)">Innexin gap junctions in nerve cells coordinate spontaneous contractile behavior in Hydra polyps.</a> Sci. Rep. 4 (3573), (2014).</li>
<li>Marcum, B. A. Culturing Epithelial Hydra. <a target="_blank" href="http://scholar.google.com/scholar?hl=en&safe=off&q=author%3aMarcum%2C+BA+%22Hydra%3A+Research+Methods%22">Hydra: Research Methods</a>. , Plenum Press. New York. 287-290 (1983).</li>
<li>David, C. N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((A+quantitative+method+for+maceration+of+Hydra+tissue%5BTitle%5D)+AND+%22Wilhelm+Roux+Arch.+Entwickl.+Mech.+Org%22%5BJournal%5D)">A quantitative method for maceration of Hydra tissue.</a> Wilhelm Roux Arch. Entwickl. Mech. Org. 171, 259-268 (1973).</li>
<li>Gröger, H., Schmid, V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Larval+development+in+Cnidaria%3A+A+connection+to+Bilateria%5BTitle%5D)+AND+%22Genesis%22%5BJournal%5D)">Larval development in Cnidaria: A connection to Bilateria.</a> Genesis. 29 (3), 110-114 (2001).</li>
<li>Lenhoff, H. M. Water, Culture Solutions, and Buffers. <a target="_blank" href="http://scholar.google.com/scholar?hl=en&safe=off&q=author%3aLenhoff%2C+HM+%22Hydra%3A+Research+Methods%22">Hydra: Research Methods</a>. , Plenum Press. New York. 29-34 (1983).</li>
<li>Shenk, M. A., Bode, H. R., Steele, R. E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Expression+of+Cnox-2%2C+a+HOM%2FHOX+homeobox+gene+in+hydra%2C+is+correlated+with+axial+pattern+formation%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">Expression of Cnox-2, a HOM/HOX homeobox gene in hydra, is correlated with axial pattern formation.</a> Development. 117, 657-667 (1993).</li>
<li>Böttger, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Horizontal+Gene+Transfer+Contributed+to+the+Evolution+of+Extracellular+Surface+Structures%3A+The+Freshwater+Polyp+Hydra+Is+Covered+by+a+Complex+Fibrous+Cuticle+Containing+Glycosaminoglycans+and+Proteins+of+the+PPOD+and+SWT+%28Sweet+Tooth%29+Families%5BTitle%5D)+AND+%22PLoS+One%22%5BJournal%5D)">Horizontal Gene Transfer Contributed to the Evolution of Extracellular Surface Structures: The Freshwater Polyp Hydra Is Covered by a Complex Fibrous Cuticle Containing Glycosaminoglycans and Proteins of the PPOD and SWT (Sweet Tooth) Families.</a> PLoS One. 7 (12), (2012).</li>
<li>King, R. S., Newmark, P. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((In+situ+hybridization+protocol+for+enhanced+detection+of+gene+expression+in+the+planarian+Schmidtea+mediterranea%5BTitle%5D)+AND+%22BMC+Dev.+Biol%22%5BJournal%5D)">In situ hybridization protocol for enhanced detection of gene expression in the planarian Schmidtea mediterranea.</a> BMC Dev. Biol. 13 (8), (2013).</li>
</ol>

The authors have nothing to disclose.

Hydra interstitial cells can be eliminated through a double colchicine treatment3,4. In the days following the first treatment, it is critical to prevent contact between individual Hydra to avoid fusion of Hydra pieces into deformed Hydra. Also, animals that can eat unassisted following the first treatment must be removed as the second colchicine treatment may not be sufficient to eliminate the remaining interstitial cells from...

The nervous system of Hydra consists of a nerve net, with neurons associated with both epithelial tissue layers1. The nerve net is denser in the hypostome and peduncle and less dense in the body column2. The nerve cells originate from interstitial stem cells, which are multipotent stem cells that give rise to secretory cells, nematocytes, germ cells, and neurons1. It is possible to eliminate the interstitial cells of Hydra vulgaris through treatment with colchicine3,4, a plant-derived toxin that kills dividing cells. Although colchicine has been found to inhibit microtubule polymerization in other organisms, a previous study has shown that microtubules are present in Hydra throughout the entire treatment, suggesting that colchicine does not act this way in Hydra3. Another study suggests that colchicine does not bind efficiently to tubulin in some organisms, including Tetrahymena pyriformis, Zea mays, Chlamydomonas, and Schizosaccharomyces pombe, which may explain this difference5. The colchicine treatment induces phagocytosis of the interstitial cells by the endodermal epithelial cells3 and thus allows for the creation of animals that are lacking nerve cells, gland cells, and nematocytes. It is unclear why the interstitial cells are particularly susceptible to colchicine treatment. Given that both post-mitotic interstitial cells and the interstitial stem cell lineage are damaged and phagocytosed, Campbell concluded that colchicine was not directly affecting mitotic activity3. Notably, the colchicine treatment works well in Hydra vulgaris, but has been shown to not work as well in other species, such as Hydra oligactis6. A modified treatment with colchicine and hydroxyurea can be used to produce nerve-free Hydra viridis7. Nerve-free Hydra (also sometimes referred to as &#34;epithelial Hydra&#34;8) are therefore a useful tool for studying the roles of these specialized cell types from the interstitial cell lineage in tissue homeostasis and regeneration.
Hydra may be the only known example of an animal capable of living without a nervous system. Nerve-free Hydra serve as a particularly useful model for dissecting the role of the nerve net in regulating Hydra regeneration, homeostasis, and behavior. For example, the introduction of interstitial cells into nerve-free Hydra via grafting allowed for the characterization of nerve cell differentiation as highly region-specific9. Furthermore, because nerve-free Hydra can regenerate, they enable the investigation of alternative, nervous system-independent regeneration pathways. One such example is apical neurogenesis and head formation, which has been shown to depend on cnox-2 function in the nervous system in wildtype Hydra, but appears to be dispensable in nerve-free Hydra, suggesting that there may be an alternative head regeneration process10.
Nerve-free Hydra have also been used to study epithelial cell expression and regulation of neurogenic and neurotransmission genes after the loss of neurogenesis11. Nerve-free Hydra do not exhibit spontaneous contraction bursts12, indicating that these bursts are regulated by the nervous system. Nerve-free Hydra do, however, contract in response to pinching the body column with forceps, suggesting that contraction in response to mechanical stimuli is mediated by coupling through gap junctions in epithelial cells, while spontaneous contractile behavior is mediated by coupling through gap junctions in nerve cells13.
Nerve-free Hydra do not open their mouths when presented with food or reduced glutathione3, suggesting that sensory neurons are necessary to detect the presence of food and signal the mouth to open. In addition, the nerve net seems to play a role in sensing osmotic pressure, because nerve-free animals are unable to autonomously regulate their internal hydrostatic pressure through mouth opening, causing their characteristic balloon-like appearance3,4 (Figure 1B). Regulation of hydrostatic pressure in nerve-free Hydra by frequent manual deflation led to a loss of some abnormal morphology in the hypostome and body column. However, chronic deflation led to interference with growth, elongation, budding, and tissue organization8.
Although nerve-free Hydra are unable to feed and egest on their own, it is possible to maintain them indefinitely in the laboratory by manually force-feeding and burping each animal. Previous publications have described methods of force-feeding and burping nerve-free Hydra, however these protocols involved the use of micropipette tips that must be hand pulled carefully to the appropriate size as well as use of a mouthpiece connected to the pipette by tubing14. Here, a simpler, safer, and more time-efficient method of feeding and burping is described.
In addition, previous studies involved checking for the absence of nerve cells through dissociation of fixed animals into individual cells and examination of cell morphology3,4,15. Here, immunohistochemistry with a monoclonal antibody against the tyrosinated carboxyl-terminus of alpha-tubulin was used as a complimentary method to maceration to check for the depletion of neurons in the hypostome13,16. Previous studies have shown that neurons in the peduncle can also be visualized using this antibody13, however these neurons as well as those in the body column are more difficult to make out. While immunohistochemistry is sufficient to confirm the absence of nerve cells in the hypostome and does not require expertise on cell type morphology, it cannot be used to check for the absence of the interstitial stem cells and the other derivatives of these cells. Dissociation and cell morphology studies are more rigorous and can give a quantitative account of the numbers of each cell type remaining following each stage of the treatment.

<table><tbody><tr><td>Colchicine</td><td>Acros Organics</td><td>227120010</td><td></td></tr><tr><td>1 mL Syringe</td><td>BD</td><td>301025</td><td></td></tr><tr><td>Brine Shrimp Eggs</td><td>Brine Shrimp Direct</td><td>N/A</td><td>Can be purchased locally</td></tr><tr><td>Brine Shrimp Hatchery Dish</td><td>Brine Shrimp Direct</td><td>N/A</td><td></td></tr><tr><td>60 mm x 15 mm Petri Dish</td><td>Celltreat</td><td>229663</td><td></td></tr><tr><td>30 G x 3/4&quot; Hypodermic Needle</td><td>Covidien</td><td>1188830340</td><td>A 27G needle may also be used</td></tr><tr><td>2 x Fine-tip Tweezers</td><td>Dumont</td><td>0109-5-PO</td><td></td></tr><tr><td>Rifampicin</td><td>EMD Millipore</td><td>557303</td><td></td></tr><tr><td>Goat anti-mouse lgG, Pab (HRP Conjugate)</td><td>Enzo</td><td>ADI-SAB-100-J</td><td></td></tr><tr><td>Bovine Serum Albumin (BSA)</td><td>Fisher</td><td>BP9703-100</td><td></td></tr><tr><td>Scalpel</td><td>Fisher</td><td>08-920A</td><td></td></tr><tr><td>Fetal Bovine Serum (FBS)</td><td>Gibco</td><td>10437028</td><td></td></tr><tr><td>DAPI (4&#039;,6-Diamidino-2-Phenylindole, Dihydrochloride)</td><td>Invitrogen</td><td>D1306</td><td></td></tr><tr><td>PBS Tablets</td><td>MP Bio</td><td>2810305</td><td></td></tr><tr><td>Monoclonal Anti-Tubulin, Tyrosine</td><td>Sigma</td><td>T9028</td><td></td></tr><tr><td>Dimethyl Sulfoxide (DMSO)</td><td>Sigma</td><td>D2650</td><td></td></tr><tr><td>Hydrogen Peroxide</td><td>Sigma</td><td>216763</td><td></td></tr><tr><td>Paraformaldehyde (PFA)</td><td>Sigma</td><td>P6148</td><td></td></tr><tr><td>Triton X - 100</td><td>Sigma</td><td>T9284</td><td></td></tr><tr><td>Tween 20</td><td>Sigma</td><td>P1379</td><td></td></tr><tr><td>Urethane</td><td>Sigma</td><td>U2500</td><td></td></tr><tr><td>Air Pump</td><td>Tetra</td><td>77846-00</td><td></td></tr><tr><td>Glass Pasteur Pipette</td><td>VWR</td><td>53283-916</td><td>Length of the pipet does not matter</td></tr><tr><td>15 mL Tube</td><td>VWR</td><td>89039-670</td><td></td></tr><tr><td>P320 Sandpaper</td><td>3M</td><td>IBGABBV00397</td><td>Can be purchased at local home improvement store</td></tr></tbody></table>

generation and long-term maintenance of nerve-free hydra

The interstitial cell lineage of Hydra includes multipotent stem cells, and their derivatives: gland cells, nematocytes, germ cells, and nerve cells. The interstitial cells can be eliminated through two consecutive treatments with colchicine, a plant-derived toxin that kills dividing cells, thus erasing the potential for renewal of the differentiated cells that are derived from the interstitial stem cells. This allows for the generation of Hydra that lack nerve cells. A nerve-free polyp cannot open its mouth to feed, egest, or regulate osmotic pressure. Such animals, however, can survive and be cultured indefinitely in the laboratory if regularly force-fed and burped. The lack of nerve cells allows for studies of the role of the nervous system in regulating animal behavior and regeneration. Previously published protocols for nerve-free Hydra maintenance involve outdated techniques such as mouth-pipetting with hand-pulled micropipette tips to feed and clean the Hydra. Here, an improved protocol for maintenance of nerve-free Hydra is introduced. Fine-tipped forceps are used to force open the mouth and insert freshly killed Artemia. Following force-feeding, the body cavity of the animal is flushed with fresh medium using a syringe and hypodermic needle to remove undigested material, referred to here as "burping". This new method of force-feeding and burping nerve-free Hydra through the use of forceps and syringes eliminates the need for mouth-pipetting using hand-pulled micropipette tips. It thus makes the process safer and significantly more time efficient. To ensure that the nerve cells in the hypostome have been eliminated, immunohistochemistry using anti-tyrosine-tubulin is conducted.

Immediately following the initial 8 h colchicine treatment, all Hydra survive. Some of these Hydra will have only tentacle stubs remaining (Figure 3A), while others will have completely lost their tentacles (Figure 3B). Over the following 1 or 2 days, the tentacles will continue to shrink until all Hydra have lost their tentacles. About 1 week following the treatment, t...

Watch this Scientific Journal Video about Generation and Long-term Maintenance of Nerve-free Hydra at JoVE.com

Generation and Long-term Maintenance of Nerve-free Hydra

Through a double treatment with colchicine, a plant-derived toxin that kills dividing cells, nerve-free Hydra vulgaris can be generated. These Hydra cannot feed or egest on their own. This paper describes an improved method for long-term maintenance of nerve free Hydra vulgaris in the laboratory.

Generation and Long-term Maintenance of Nerve-free Hydra

The interstitial cell lineage of Hydra includes multipotent stem cells, and their derivatives: gland cells, nematocytes, germ cells, and nerve cells. The ...

generation-and-long-term-maintenance-of-nerve-free-hydra

Research

JoVE Journal

Neuroscience

12.5K Views.  UC San Diego. Through a double treatment with colchicine, a plant-derived toxin that kills dividing cells, nerve-free Hydra vulgaris can be generated. These Hydra cannot feed or egest on their own. This paper describes an improved method for long-term maintenance of nerve free Hydra vulgaris in the laboratory.

Video: Generation and Long-term Maintenance of Nerve-free Hydra

Inducing Complete Polyp Regeneration from the Aboral Physa of the Starlet Sea Anemone Nematostella vectensis

Cnidarians, and specifically Hydra, were the first animals shown to regenerate damaged or severed structures, and indeed such studies arguably launched modern biological inquiry through the work of Trembley more than 250 years ago. Presently the study of regeneration has seen a resurgence using both &#34;classic&#34; regenerative organisms, such as the Hydra, planaria and Urodeles, as well as a widening spectrum of species spanning the range of metazoa, from sponges through mammals. Besides its intrinsic interest as a biological phenomenon, understanding how regeneration works in a variety of species will inform us about whether regenerative processes share common features and/or species or context-specific cellular and molecular mechanisms. The starlet sea anemone, Nematostella vectensis, is an emerging model organism for regeneration. Like Hydra, Nematostella is a member of the ancient phylum, cnidaria, but within the class anthozoa, a sister clade to the hydrozoa that is evolutionarily more basal. Thus aspects of regeneration in Nematostella will be interesting to compare and contrast with those of Hydra and other cnidarians. In this article, we present a method to bisect, observe and classify regeneration of the aboral end of the Nematostella adult, which is called the physa. The physa naturally undergoes fission as a means of asexual reproduction, and either natural fission or manual amputation of the physa triggers re-growth and reformation of complex morphologies. Here we have codified these simple morphological changes in a Nematostella Regeneration Staging System (the NRSS). We use the NRSS to test the effects of chloroquine, an inhibitor of lysosomal function that blocks autophagy. The results show that the regeneration of polyp structures, particularly the mesenteries, is abnormal when autophagy is inhibited.

Inducing Complete Polyp Regeneration from the Aboral Physa of the Starlet Sea Anemone Nematostella vectensis

Here we demonstrate how to induce and monitor regeneration in the Starlet Sea Anemone Nematostella vectensis, a model cnidarian anthozoan. We demonstrate how to amputate and categorize regeneration using a morphological staging system, and we use this system to reveal a requirement for autophagy in regenerating polyp structures.

Cnidarians, and specifically Hydra, were the first animals shown to regenerate damaged or severed structures, and indeed such studies arguably launched ...

Developmental Biology

Genetic Study of Axon Regeneration with Cultured Adult Dorsal Root Ganglion Neurons

It is well known that mature neurons in the central nervous system (CNS) cannot regenerate their axons after injuries due to diminished intrinsic ability to support axon growth and a hostile environment in the mature CNS1,2. In contrast, mature neurons in the peripheral nervous system (PNS) regenerate readily after injuries3. Adult dorsal root ganglion (DRG) neurons are well known to regenerate robustly after peripheral nerve injuries. Each DRG neuron grows one axon from the cell soma, which branches into two axonal branches: a peripheral branch innervating peripheral targets and a central branch extending into the spinal cord. Injury of the DRG peripheral axons results in substantial axon regeneration, whereas central axons in the spinal cord regenerate poorly after the injury. However, if the peripheral axonal injury occurs prior to the spinal cord injury (a process called the conditioning lesion), regeneration of central axons is greatly improved4. Moreover, the central axons of DRG neurons share the same hostile environment as descending corticospinal axons in the spinal cord. Together, it is hypothesized that the molecular mechanisms controlling axon regeneration of adult DRG neurons can be harnessed to enhance CNS axon regeneration. As a result, adult DRG neurons are now widely used as a model system to study regenerative axon growth5-7.
Here we describe a method of adult DRG neuron culture that can be used for genetic study of axon regeneration in vitro. In this model adult DRG neurons are genetically manipulated via electroporation-mediated gene transfection6,8. By transfecting neurons with DNA plasmid or si/shRNA, this approach enables both gain- and loss-of-function experiments to investigate the role of any gene-of-interest in axon growth from adult DRG neurons. When neurons are transfected with si/shRNA, the targeted endogenous protein is usually depleted after 3-4 days in culture, during which time robust axon growth has already occurred, making the loss-of-function studies less effective. To solve this problem, the method described here includes a re-suspension and re-plating step after transfection, which allows axons to re-grow from neurons in the absence of the targeted protein. Finally, we provide an example of using this in vitro model to study the role of an axon regeneration-associated gene, c-Jun, in mediating axon growth from adult DRG neurons9.

An in vitro model for genetic study of axon regeneration using cultured adult mouse dorsal root ganglion neurons is described. The method includes a re-suspension/re-plating step to allow axon re-growth from neurons undergoing genetic manipulation. This approach is especially useful for loss-of-function studies of axon regeneration using RNAi-based protein knockdown.

It is well known that mature neurons in the central nervous system (CNS) cannot regenerate their axons after injuries due to diminished intrinsic ability ...

Motor Nerve Transection and Time-lapse Imaging of Glial Cell Behaviors in Live Zebrafish

The nervous system is often described as a hard-wired component of the body even though it is a considerably fluid organ system that reacts to external stimuli in a consistent, stereotyped manner, while maintaining incredible flexibility and plasticity. Unlike the central nervous system (CNS), the peripheral nervous system (PNS) is capable of significant repair, but we have only just begun to understand the cellular and molecular mechanisms that govern this phenomenon. Using zebrafish as a model system, we have the unprecedented opportunity to couple regenerative studies with in vivo imaging and genetic manipulation. Peripheral nerves are composed of axons surrounded by layers of glia and connective tissue. Axons are ensheathed by myelinating or non-myelinating Schwann cells, which are in turn wrapped into a fascicle by a cellular sheath called the perineurium. Following an injury, adult peripheral nerves have the remarkable capacity to remove damaged axonal debris and re-innervate targets. To investigate the roles of all peripheral glia in PNS regeneration, we describe here an axon transection assay that uses a commercially available nitrogen-pumped dye laser to axotomize motor nerves in live transgenic zebrafish. We further describe the methods to couple these experiments to time-lapse imaging of injured and control nerves. This experimental paradigm can be used to not only assess the role that glia play in nerve regeneration, but can also be the platform for elucidating the molecular mechanisms that govern nervous system repair.

Although the peripheral nervous system (PNS) is capable of significant repair after injury, little is known about the cellular and molecular mechanisms that govern this phenomenon. Using live, transgenic zebrafish and a reproducible nerve transection assay, we can study dynamic glial cell behaviors during nerve degeneration and regeneration.

The  nervous system is often described as a hard-wired component of the body even  though it is a considerably fluid organ system that reacts to external ...

Three-dimensional Tissue Engineered Aligned Astrocyte Networks to Recapitulate Developmental Mechanisms and Facilitate Nervous System Regeneration

Neurotrauma and neurodegenerative disease often result in lasting neurological deficits due to the limited capacity of the central nervous system (CNS) to replace lost neurons and regenerate axonal pathways. However, during nervous system development, neuronal migration and axonal extension often occur along pathways formed by other cells, referred to as &#34;living scaffolds&#34;. Seeking to emulate these mechanisms and to design a strategy that circumvents the inhibitory environment of the CNS, this manuscript presents a protocol to fabricate tissue engineered astrocyte-based &#34;living scaffolds&#34;. To create these constructs, we employed a novel biomaterial encasement scheme to induce astrocytes to self-assemble into dense three-dimensional bundles of bipolar longitudinally-aligned somata and processes. First, hollow hydrogel micro-columns were assembled, and the inner lumen was coated with collagen extracellular-matrix. Dissociated cerebral cortical astrocytes were then delivered into the lumen of the cylindrical micro-column and, at a critical inner diameter of &#60;350 &#181;m, spontaneously self-aligned and contracted to produce long fiber-like cables consisting of dense bundles of astrocyte processes and collagen fibrils measuring &#60;150 &#181;m in diameter yet extending several cm in length. These engineered living scaffolds exhibited &#62;97% cell viability and were virtually exclusively comprised of astrocytes expressing a combination of the intermediate filament proteins glial-fibrillary acidic protein (GFAP), vimentin, and nestin. These aligned astrocyte networks were found to provide a permissive substrate for neuronal attachment and aligned neurite extension. Moreover, these constructs maintain integrity and alignment when extracted from the hydrogel encasement, making them suitable for CNS implantation. These preformed constructs structurally emulate key cytoarchitectural elements of naturally occurring glial-based &#34;living scaffolds&#34; in vivo. As such, these engineered living scaffolds may serve as test-beds to study neurodevelopmental mechanisms in vitro or facilitate neuroregeneration by directing neuronal migration and/or axonal pathfinding following CNS degeneration in vivo.

We showcase the development of self-assembled, three-dimensional bundles of longitudinally aligned astrocytic somata and processes within a novel biomaterial encasement. These engineered &#34;living scaffolds&#34;, exhibiting micron-scale diameter yet extending centimeters in length, may serve as test-beds to study neurodevelopmental mechanisms or facilitate neuroregeneration by directing neuronal migration and/or axonal pathfinding.

Neurotrauma and neurodegenerative disease often result in lasting neurological deficits due to the limited capacity of the central nervous system (CNS) to ...

Bioengineering

Fluorescent In Situ Hybridization and 5-Ethynyl-2'-Deoxyuridine Labeling for Stem-Like Cells in the Hydrozoan Jellyfish Cladonema pacificum

Cnidarians, including sea anemones, corals, and jellyfish, exhibit diverse morphology and lifestyles that are manifested in sessile polyps and free-swimming medusae. As exemplified in established models such as Hydra and Nematostella, stem cells and/or proliferative cells contribute to the development and regeneration of cnidarian polyps. However, the underlying cellular mechanisms in most jellyfish, particularly at the medusa stage, are largely unclear, and, thus, developing a robust method for identifying specific cell types is critical. This paper describes a protocol for visualizing stem-like proliferating cells in the hydrozoan jellyfish Cladonema pacificum. Cladonema medusae possess branched tentacles that continuously grow and maintain regenerative capacity throughout their adult stage, providing a unique platform with which to study the cellular mechanisms orchestrated by proliferating and/or stem-like cells. Whole-mount fluorescent in situ hybridization (FISH) using a stem cell marker allows for the detection of stem-like cells, while pulse labeling with 5-ethynyl-2&#39;-deoxyuridine (EdU), an S phase marker, enables the identification of proliferating cells. Combining both FISH and EdU labeling, we can detect actively proliferating stem-like cells on fixed animals, and this technique can be broadly applied to other animals, including non-model jellyfish species.

Fluorescent In Situ Hybridization and 5-Ethynyl-2'-Deoxyuridine Labeling for Stem-Like Cells in the Hydrozoan Jellyfish Cladonema pacificum

Here, we describe a protocol for visualizing stem-like proliferating cells in the jellyfish Cladonema. Whole-mount fluorescent in situ hybridization with a stem cell marker allows for the detection of stem-like cells, and 5-ethynyl-2&#39;-deoxyuridine labeling enables the identification of proliferating cells. Together, actively proliferating stem-like cells can be detected.&#160;

Cnidarians, including sea anemones, corals, and jellyfish, exhibit diverse morphology and lifestyles that are manifested in sessile polyps and ...

Anatomically Inspired Three-dimensional Micro-tissue Engineered Neural Networks for Nervous System Reconstruction, Modulation, and Modeling

Functional recovery rarely occurs&#160;following injury or disease-induced degeneration within the central nervous system (CNS)&#160;due to the inhibitory environment and the limited capacity for neurogenesis. We are developing&#160;a strategy to simultaneously address&#160;neuronal and axonal pathway loss within the damaged CNS. This manuscript presents the fabrication protocol for micro-tissue engineered neural networks (micro-TENNs), implantable constructs consisting of neurons and aligned axonal tracts spanning the extracellular matrix (ECM) lumen of a preformed hydrogel cylinder hundreds of microns in diameter that may extend centimeters in length. Neuronal aggregates are delimited to the extremes of the three-dimensional encasement and are spanned by axonal projections. Micro-TENNs are uniquely poised as a strategy for CNS reconstruction, emulating aspects of brain connectome cytoarchitecture and potentially providing means for network replacement. The neuronal aggregates may synapse with host tissue to form new functional relays to restore and/or modulate missing or damaged circuitry. These constructs may also act as pro-regenerative&#160;&#34;living scaffolds&#34; capable of exploiting developmental mechanisms for cell migration and axonal pathfinding, providing synergistic structural and soluble cues based on the state of regeneration. Micro-TENNs are fabricated by pouring liquid hydrogel into a cylindrical mold containing a longitudinally centered needle. Once the hydrogel has gelled, the needle is removed, leaving a hollow micro-column. An ECM solution is added to the lumen to provide an environment suitable for neuronal adhesion and axonal outgrowth. Dissociated neurons are mechanically aggregated for precise seeding within one or both ends of the micro-column. This methodology reliably produces self-contained miniature constructs with long-projecting axonal tracts that may recapitulate features of brain neuroanatomy. Synaptic immunolabeling and genetically encoded calcium indicators suggest that micro-TENNs possess extensive synaptic distribution and intrinsic electrical activity. Consequently, micro-TENNs represent a promising strategy for targeted neurosurgical reconstruction of brain pathways and may also be applied as biofidelic models to study neurobiological phenomena in vitro.

This manuscript details the fabrication of micro-tissue engineered neural networks: three-dimensional micron-sized constructs comprised of long aligned axonal tracts spanning aggregated neuronal population(s) encased in a tubular hydrogel. These living scaffolds can serve as functional relays to reconstruct or modulate neural circuitry or as biofidelic test-beds mimicking gray-white matter neuroanatomy.

Functional recovery rarely occurs&#160;following injury or disease-induced degeneration within the central nervous system (CNS)&#160;due to the inhibitory ...

Rewiring Neuronal Circuits: A New Method for Fast Neurite Extension and Functional Neuronal Connection

Brain and spinal cord injury may lead to permanent disability and death because it is still not possible to regenerate neurons over long distances and accurately reconnect them with an appropriate target. Here a procedure is described to rapidly initiate, elongate, and precisely connect new functional neuronal circuits over long distances. The extension rates achieved reach over 1.2 mm/h, 30-60 times faster than the in vivo rates of the fastest growing axons from the peripheral nervous system (0.02 to 0.04 mm/h)28 and 10 times faster than previously reported for the same neuronal type at an earlier stage of development4. First, isolated populations of rat hippocampal neurons are grown for 2-3 weeks in microfluidic devices to precisely position the cells, enabling easy micromanipulation and experimental reproducibility. Next, beads coated with poly-D-lysine (PDL) are placed on neurites to form adhesive contacts and pipette micromanipulation is used to move the resulting bead-neurite complex. As the bead is moved, it pulls out a new neurite that can be extended over hundreds of micrometers and functionally connected to a target cell in less than 1 h. This process enables experimental reproducibility and ease of manipulation while bypassing slower chemical strategies to induce neurite growth. Preliminary measurements presented here demonstrate a neuronal growth rate far exceeding physiological ones. Combining these innovations allows for the precise establishment of neuronal networks in culture with an unprecedented degree of control. It is a novel method that opens the door to a plethora of information and insights into signal transmission and communication within the neuronal network as well as being a playground in which to explore the limits of neuronal growth. The potential applications and experiments are widespread with direct implications for therapies that aim to reconnect neuronal circuits after trauma or in neurodegenerative diseases.

This procedure describes how to rapidly initiate, extend and connect neurites organized in microfluidic chambers using poly-D-lysine-coated beads fixed to micropipettes that guide neurite elongation.

Brain and spinal cord injury may lead to permanent disability and death because it is still not possible to regenerate neurons over long distances and ...

Generation of Neurospheres from Mixed Primary Hippocampal and Cortical Neurons Isolated from E14-E16 Sprague Dawley Rat Embryo

Primary neuron culture is an essential technique in the field of neuroscience. To gain deeper mechanistic insights into the brain, it is essential to have a robust in vitro model that can be exploited for various neurobiology studies. Though primary neuron cultures (i.e., long-term hippocampal cultures) have provided scientists with models, it does not yet represent the complexity of brain network completely. In the wake of these limitations, a new model has emerged using neurospheres, which bears a closer resemblance to the brain tissue. The present protocol describes the plating of high and low densities of mixed cortical and hippocampal neurons isolated from the embryo of embryonic day 14-16 Sprague Dawley rats. This allows for the generation of neurospheres and long-term primary neuron culture as two independent platforms to conduct further studies. This process is extremely simple and cost-effective, as it minimizes several steps and reagents previously deemed essential for neuron culture. This is a robust protocol with minimal requirements that can be performed with achievable results and further used for a diversity of studies related to neuroscience.

Presented here is a protocol for the spontaneous generation of neurospheres enriched in neural progenitor cells from high density plated neurons. During the same experiment, when neurons are plated at a lower density, the protocol also results in prolonged primary rat neuron cultures.

Primary neuron culture is an essential technique in the field of neuroscience. To gain deeper mechanistic insights into the brain, it is essential to have ...

Generation of Transgenic Hydra by Embryo Microinjection

As a member of the phylum Cnidaria, the sister group to all bilaterians, Hydra can shed light on fundamental biological processes shared among multicellular animals. Hydra is used as a model for the study of regeneration, pattern formation, and stem cells. However, research efforts have been hampered by lack of a reliable method for gene perturbations to study molecular function. The development of transgenic methods has revitalized the study of Hydra biology1. Transgenic Hydra allow for the tracking of live cells, sorting to yield pure cell populations for biochemical analysis, manipulation of gene function by knockdown and over-expression, and analysis of promoter function. Plasmid DNA injected into early stage embryos randomly integrates into the genome early in development. This results in hatchlings that express transgenes in patches of tissue in one or more of the three lineages (ectodermal epithelial, endodermal epithelial, or interstitial). The success rate of obtaining a hatchling with transgenic tissue is between 10% and 20%. Asexual propagation of the transgenic hatchling is used to establish a uniformly transgenic line in a particular lineage. Generating transgenic Hydra is surprisingly simple and robust, and here we describe a protocol that can be easily implemented at low cost.

Generation of Transgenic Hydra by Embryo Microinjection

Stably transgenic Hydra are made by microinjection of plasmid DNA into embryos followed by random genomic integration and asexual propagation to establish a uniform line. Transgenic Hydra are used to track cell movements, overexpress genes, study promoter function, or knock down gene expression using RNAi.

As a member of the phylum Cnidaria, the sister group to all bilaterians, Hydra can shed light on fundamental biological processes shared among ...

Biology

Efficient Nucleofection of NSCs Isolated from the Murine Subventricular Zone

Isolation, Expansion, and Nucleofection of Neural Stem Cells from Adult Murine Subventricular Zone

Isolation and expansion of neural stem cells (NSCs) from the subventricular zone (SVZ) of the adult mouse brain can be achieved in a medium supplemented with basic fibroblast growth factor (bFGF) and epidermal growth factor (EGF) as mitogens, producing clonal aggregates known as neurospheres. This in vitro system is a valuable tool for studying NSC potential. Transfection of siRNAs or genes carried in plasmids can be used to induce perturbations to gene expression and study NSC biology. However, the exogenous nucleic acid delivery to NSC cultures is challenging due to the low efficiency of central nervous system (CNS) cells transfection. Here, we present an improved nucleofection system that achieves high efficiency of gene delivery in expanded NSCs from adult murine SVZ. We demonstrate that this relatively simple method enhances gene perturbation in adult NSCs, surpassing traditional transfection protocols with survival rates exceeding 80%. Moreover, this method can also be applied in primary isolated NSCs, providing a crucial advancement in gene function studies through gene expression manipulation via knockdown or overexpression in neurosphere cultures.

Author Spotlight: Improved Nucleofection for High-Efficiency Gene Delivery in Murine Subventricular Zone-Derived Neural Stem Cell Cultures

Here, we describe a nucleofection system designed to enhance gene delivery efficiency in expanded neural stem cells (NSCs) isolated from the adult murine subventricular zone. The findings demonstrate that this method significantly improves gene perturbation in NSCs, surpassing the effectiveness of traditional transfection protocols and enhancing cell survival rate.

Isolation and expansion of neural stem cells (NSCs) from the subventricular zone (SVZ) of the adult mouse brain can be achieved in a medium supplemented ...

Generation and Long-term Maintenance of Nerve-free Hydra

Summary

Explore More Videos

Inducing Complete Polyp Regeneration from the Aboral Physa of the Starlet Sea Anemone Nematostella vectensis

Genetic Study of Axon Regeneration with Cultured Adult Dorsal Root Ganglion Neurons

Motor Nerve Transection and Time-lapse Imaging of Glial Cell Behaviors in Live Zebrafish

Three-dimensional Tissue Engineered Aligned Astrocyte Networks to Recapitulate Developmental Mechanisms and Facilitate Nervous System Regeneration

Fluorescent In Situ Hybridization and 5-Ethynyl-2'-Deoxyuridine Labeling for Stem-Like Cells in the Hydrozoan Jellyfish Cladonema pacificum

Anatomically Inspired Three-dimensional Micro-tissue Engineered Neural Networks for Nervous System Reconstruction, Modulation, and Modeling

Rewiring Neuronal Circuits: A New Method for Fast Neurite Extension and Functional Neuronal Connection

Generation of Neurospheres from Mixed Primary Hippocampal and Cortical Neurons Isolated from E14-E16 Sprague Dawley Rat Embryo

Generation of Transgenic Hydra by Embryo Microinjection

Isolation, Expansion, and Nucleofection of Neural Stem Cells from Adult Murine Subventricular Zone