The authors received no specific funding for this work. Professor Maria Grazia Cappai and Dr. Valeria Pasciu are gratefully acknowledged for the video voiceover and for setting up the lab during the video making.

The animal protocol and the implemented procedures described below are in accordance with the ethical guidelines in force at the University of Sassari, in compliance with the European Union Directive 86/609/EC and the recommendation of the Commission of the European Communities 2007/526/EC.
1. Preparation of media for oocyte manipulation
<ol>
	<li>Prepare the medium for transport of collected ovaries by supplementing Dulbecco&#39;s phosphate buffered saline with 0.1 g/L penicillin and 0.1 g/L streptomycin (PBS).</li>
	<li>Prepare the medium for oocyte collection and maturation by diluting 9.5 g of Tissue Culture Medium (TCM) 199 in powder with 1 L of Milli-Q water supplemented with penicillin (0.1%) and streptomycin (0.1%).
	<ol>
		<li>After dilution, filter 100 mL of medium and store it at 4 &#176;C as Stock Maturation Medium (SMM) to be used for one week.</li>
		<li>Prepare the collection medium (CM) by supplementing the remaining 900 mL with 25 mM HEPES, 0.36 g/L bicarbonate and 0.1% (w/v) polyvinyl alcohol (PVA) (pH 7.3, osmolality 290 mOsm/kg).</li>
	</ol>
	</li>
	<li>Prepare the maturation medium with SMM supplemented with 0.021 g/L bicarbonate, 10% heat-treated estrus sheep serum, 1 IU/mL FSH, 1 IU/mL LH, 100 &#181;L of cysteamine and 8 mg/mL of pyruvate. 
	NOTE: The maturation medium in a volume of 10 mL must be incubated at standard conditions (in a maximum humidified atmosphere at 39 &#176;C in 5% CO2 in air) for at least 4 h before use.</li>
	<li>Prepare the base medium (BM) for manipulation of oocyte after in vitro maturation, consisting in PBS without Ca++ and Mg++, supplemented with 20% fetal calf serum (FCS).</li>
</ol>
2. Oocyte collection and maturation
<ol>
	<li>Recover the oocytes from juvenile (30-40 days of age, body weight 6-10 kg) and adult ovaries.</li>
	<li>Transport the collected ovaries from the commercial slaughterhouse to the laboratory within 1-2 h in PBS at 27 &#176;C.</li>
	<li>After washing in PBS fresh medium, slice the ovaries in CM using a micro-blade to release the follicle content.</li>
	<li>Under a stereomicroscope examination with 60x magnification, select cumulus-oocyte complexes (COCs) for in vitro maturation by choosing those with 4-10 layers of granulosa cells, oocyte with a uniform cytoplasm, homogeneous distribution of lipid droplets in the cytoplasm and with the outer diameter of about 90 &#181;m (mean).</li>
	<li>Wash the selected COCs three times in CM and finally transfer them in maturation medium. 
	NOTE: For juvenile oocytes, to improve survival after vitrification, supplement the maturation medium with 100 &#181;M trehalose.</li>
	<li>For in vitro maturation, transfer 30-35 COCs in 600 &#181;L of maturation medium in four-well Petri dishes, covered with 300 &#181;L of mineral oil and incubate them for 22 (adult oocytes)/24 (juvenile oocytes) h in 5% CO2 in air at 39 &#176;C.</li>
	<li>After in vitro maturation, denude COCs of cumulus cells by gently pipetting. Following the examination under a stereomicroscope with 60x magnification, select only those showing the extrusion on the first polar body, and thus at metaphase II (MII) stage, for vitrification.</li>
</ol>
3. Semen collection, freezing and thawing procedures
<ol>
	<li>Prepare the base medium for semen cryopreservation consisting in ram extender (200 mM Tris; 70 mM citric acid; 55 mM fructose; pH 7.2, osmolality 300 mOsm/kg) supplemented with egg yolk 20% (v/v).</li>
	<li>Collect the semen only during sheep breeding season (October-November).</li>
	<li>Obtain ejaculates by artificial vagina from adult rams (aged 2-5 years), maintained in an outdoor environment and fed a live-weight maintenance ration. Keep rams isolated in separate pens, but with visual contact between each other.</li>
	<li>Repeat semen collection one a week during the entire breeding season to obtain at least 8 ejaculates from each male.</li>
	<li>Transport the semen samples to the laboratory at environmental temperature within 5 min after collection and immediately process. Pool the ejaculates of two-three rams and evaluate sperm concentration spectrophotometry.</li>
	<li>After pooling, dilute the ejaculates up to 400 x 106 spermatozoa/mL with base medium for semen cryopreservation supplemented with 4% glycerol. Then cool the diluted semen to 4 &#176;C over a period of 2 h and equilibrate it for 20 min before freezing.</li>
	<li>Freeze the semen samples in pellet form (0.25 mL) on dry ice and then plunge them into liquid nitrogen.</li>
	<li>For thawing, put the pellet in a sterilized glass falcon and plunge it in a water bath for 20 s at 39 &#176;C.</li>
</ol>
4. In vitro fertilization and embryo culture
<ol>
	<li>Prepare stocks for constitution of the synthetical oviductal fluid (SOF).
	<ol>
		<li>Prepare Stock A: 99.4 mL of MilliQ-water; 6.29 g of NaCl; 0.534 g of KCl; 0.161 g of KH2PO4; 0.182 g of MgSO4 &#183;7H2O; and 0.6 mL of Sodium Lactate. Keep at 4 &#176;C for up to 3 months.</li>
		<li>Prepare Stock B: 10 mL of MilliQ-water; 0.210 g of NaHCO3; and 2-3 g of Phenol Red. Keep at 4 &#176;C for 1 month.</li>
		<li>Prepare Stock C: 10 mL of MilliQ-water; and 0.051 g of sodium pyruvate. Keep at 4 &#176;C for 1 month.</li>
		<li>Prepare Stock D: 10 mL of MilliQ-water; and 0.262 g of CaCl2 2H2O. Keep at 4 &#176;C for 1 month.</li>
		<li>Prepare 10 mL of SOF consisting of 7.630 mL of MilliQ water, 1 mL of Stock A, 1 mL of Stock B, 0.07 mL of Stock C and 0.7 mL of stock D.</li>
		<li>Prepare in vitro fertilization (IVF) medium: SOF supplemented with 2% heat-treated estrous sheep serum, 10 &#181;g/mL heparin and 1 &#181;g/mL hypoutarine (osmolality 280-290 mOsm/kg). 
		NOTE: The IVF medium in a volume of 10 mL must be incubated at standard conditions (in a maximum humidified atmosphere at 39 &#176;C in 5% CO2, 5% O2 and 90% N2) at least 4 h before use.</li>
	</ol>
	</li>
	<li>Transfer frozen/thawed semen aliquots in a sterilized glass conical tube below 1.5 mL of warmed IVF medium and incubate them for 15 min at 39 &#176;C in a humidified atmosphere at 5% CO2 in air.</li>
	<li>After incubation, the motile spermatozoa swim towards the apical portion of the liquid column. Collect the top layer and observe for sperm motility evaluation. 
	NOTE: Sperm motility parameters should be assessed using a computer-assisted sperm analysis (CASA) system with the following settings: 25 frames acquired to avoid sperm track overlapping, minimum contrast 10, minimum velocity of average path 30 &#181;m/s, and progressive motility &#62; 80% straightness. This system has a specific setup for ram sperm evaluation. For each sample, 5 &#181;L subsample of sperm suspension are loaded into a pre-warmed analysis chamber with a depth of 10 &#181;m. Sperm motility is assessed at 37 &#176;C at 40x using a phase contrast microscope and a minimum of 500 sperm per subsample should be analyzed in at least four different microscopic fields. The percentage of total motile and progressive motile sperm were evaluated. For the IVF, the percentage of progressive motile spermatozoa should be &#8805; 30%.</li>
	<li>Dilute swim-up derived motile spermatozoa at 1 x 106 spermatozoa/mL final concentration and co-incubate them with MII oocytes in 300 &#181;L of IVF medium covered with mineral oil in four-well Petri dishes.</li>
	<li>After 22 h transfer the presumptive zygotes in four-well Petri dishes containing SOF supplemented with 0.4% bovine serum albumin and essential and non-essential amino acids at oviductal concentration as reported by16 under mineral oil and culture them under standard conditions up to the blastocyst stage.</li>
	<li>At 22-, 26- and 32- h post-insemination, record the number of cleaved oocytes, showing two distinct blastomeres, by the examination under a stereomicroscope with 60x magnification.</li>
	<li>Observe the embryos daily starting from the fifth to the ninth day of culture and newly formed blastocysts should be recorded by the examination under a stereomicroscope with 60x magnification.</li>
</ol>
5. Oocyte vitrification and warming
NOTE: Perform vitrification following the method of minimum essential volume (MEV) using device cryotops17.
<ol>
	<li>Equilibrate a group of five oocytes at 38.5 &#176;C for 2 min in BM. The use of BM guarantees a low calcium concentration ([Ca2++] 2.2 mg/dL)10.</li>
	<li>Dehydrate the oocytes with a 3 min exposure to equilibration solution containing 7.5% (v/v) dimethyl sulfoxide (DMSO) and 7.5% (v/v) ethylene glycol (EG) in BM.</li>
	<li>Transfer the oocytes to the vitrification solution containing 16.5% (v/v) DMSO, 16.5% (v/v) EG and 0.5 M trehalose in BM before loading them in a cryotop device and directly plunging them into liquid nitrogen within 30 s.</li>
	<li>To warm to a biological temperature, transfer the content of each vitrification device from liquid nitrogen into 200 &#181;L drops of 1.25 M trehalose in BM for 1 min at 38.5 &#176;C, and gently stir to facilitate the mixing.</li>
	<li>To promote removal of intracellular cryoprotectants, transfer oocytes stepwise into 200 &#181;L drops of decreasing trehalose solutions (0.5 M, 0.25 M, 0.125 M trehalose in BM) for 30 s at 38.5 &#176;C before being equilibrated for 10 min at 38.5 &#176;C in BM.</li>
</ol>
6. Assessment of oocyte quality post-warming
<ol>
	<li>After warming, incubate the oocytes for 6 h in PBS without Ca++ and Mg++ plus 20% FCS (BM) in 5% CO2 in air at 38.5 &#176;C. 
	NOTE: The oocyte ability to restore biological and structural features after vitrification is in relation to the species and classes of used oocytes.</li>
	<li>Since the oocyte ability to recover cryopreservation damages is time-dependant, assess oocyte quality at different time points of in vitro culture (0 h, 2 h, 4 h, 6 h) after warming, to define the optimal time window for oocyte fertilization. 
	&#8203;NOTE: In adult sheep oocyte, the optimal time is 4 h post-warming; for prepubertal oocyte, the optimal time is 2 h post-warming.</li>
</ol>
7. Oocyte survival assessment
<ol>
	<li>Immediately after warming and for each time point of post-warming culture, morphologically evaluate oocytes using an inverted microscope with 100x magnification. 
	NOTE: Oocytes with structural alterations, such as faint cytoplasm, damage zona pellucida and/or membrane should be classified as degenerated.</li>
	<li>Validate the membrane integrity evaluation using a double differential fluorescent staining.</li>
	<li>Incubate the oocytes in 2 mL of BM containing propidium iodide (PI; 10 &#181;g/mL) and Hoechst 33342 (10 &#181;g/mL) for 5 min in 5% CO2 in air at 38.5 &#176;C.</li>
	<li>After washing three times in fresh BM, observe the oocytes under a fluorescent microscope using an excitation filter of 350 nm and emission of 460 nm for Hoechst 33342 and an excitation filter of 535 nm and emission of 617 nm for PI. 
	&#8203;NOTE: Oocytes with an intact membrane can be recognized by the blue fluorescence of colored DNA with Hoechst 33342. Oocyte with damaged membranes show a red fluorescence due to DNA staining with PI.</li>
</ol>
8. Evaluation of mitochondrial activity and ROS intracellular levels by confocal laser scanning microscopy
<ol>
	<li>Prepare the MitoTracker Red CM-H2XRos (MT-Red) probe.
	<ol>
		<li>Dilute the content of 1 vial (50 &#181;g) with 1 mL of DMSO to obtain a 1 mM solution. Keep the diluted vial in liquid nitrogen.</li>
		<li>Dilute the solution 1 mM with DMSO to obtain the 100 &#181;M stock solution and store it at -80 &#176;C in the dark.</li>
	</ol>
	</li>
	<li>Prepare 2&#8242;,7&#8242;-dichlorodihydrofluorescein diacetate (H2DCF-DA) probe.
	<ol>
		<li>Dilute the H2DCF-DA in 0.1% polyvinyl pyrrolidone (PVA)/PBS to obtain the first 100 mM solution. Keep the solution at -80 &#176;C in the dark .</li>
		<li>Dilute the first solution in 0.1% PVA/PBS to obtain the 100 &#181;M stock solution. Store it at -20 &#176;C in the dark.</li>
	</ol>
	</li>
	<li>Prepare the mounting medium (MM): for 10 mL of MM, add 5 mL of glycerol, 5 mL of PBS and 250 mg of sodium azide. Store it at -20 &#176;C until use.</li>
	<li>Incubate the oocytes for 30 min at 38.5 &#176;C in BM with 500 nM MT-Red (stock solution: 100 &#181;M in DMSO).</li>
	<li>After incubation with MT-Red probe, wash the oocytes three times in BM and incubate for 20 min in the same media containing 5 &#181;M H2DCF-DA (stock solution: 100 &#181;M in BM).</li>
	<li>After exposure to the probes, wash the oocytes in BM and fix in 2.5% glutaraldehyde/PBS for at least 15 min.</li>
	<li>After fixation, wash the oocytes three times in BM and mount on glass slides in a 4 &#181;L drop of MM with 1 mg/mL Hoechst 33342 using wax cushions to avoid compression of samples.</li>
	<li>Store slides at 4 &#176;C in the dark until evaluation.</li>
	<li>Perform the analysis of immunolabelled sections with a confocal laser scanning microscope. The microscope is equipped with Ar/He/Ne lasers, using a 40/60x oil objective. Analyze the sections by sequential excitation.</li>
	<li>For mitochondrial evaluation, observe the samples with a multiphoton laser to detect MT-Red (exposure: 579 nm; emission: 599 nm).</li>
	<li>Use an argon ions laser ray at 488 nm and the B-2 A filter (495 nm exposure and 519 nm emission) to point out the dichlorofluorescein (DCF)18.</li>
	<li>In each individual oocyte, measure MT-Red and DCF fluorescence intensities at the equatorial plane19.</li>
	<li>Maintain parameters related to fluorescence intensity at constant values during all image acquisitions (laser energy 26%, Sequential Settings 1: PMT1 gain 649-PMT2 gain 482; Sequential Setting 2: PMT1 gain 625-PMT2 gain 589; offset 0; pinhole size: 68).</li>
	<li>Perform quantitative analysis of fluorescence intensity using the Leica LAS AF Lite image analysis software package, following the procedures standardized by20.</li>
	<li>Capture the pictures once, moving on the Z axis, until reaching the equatorial plane.</li>
	<li>For each photo, transform to gray scale and turn off channel 1 (related to Hoechst blue) was turned off. Then manually draw a region of interest (ROI) on a circumscribed area, that is around the meiotic spindle. 
	NOTE: The software can automatically read the pixel average value on the channel 2 (FITC), subtracting the value of the background from it.</li>
	<li>Record the mean values of pixels and submit for statistical analysis.</li>
</ol>
9. Statistical Analyses
<ol>
	<li>Analyze the following differences: survival rates in juvenile vs adult oocytes, survival rates and developmental competence in control and trehalose-treated juvenile oocytes, survival and parthenogenetic activation rates and developmental competence of adult oocytes vitrified with different calcium concentration media, fertilization rates and embryo production in juvenile oocytes vitrified with low or high calcium concentration, active mitochondria phenotypes in juvenile vitrified oocytes during different time points of post-warming culture and parthenogenetic activation rates between adult and juvenile vitrified oocytes using the chi square test.</li>
	<li>Analyze the cleavage rate and embryo output in vitrified adult oocytes during different time points of post-warming culture, fluorescence intensity of mitochondrial activity and ROS intracellular levels in juvenile vitrified oocytes during different time points of post-warming culture by ANOVA after analysis for homogeneity of variance by Levene&#39;s test. Use a post-hoc test Tukey&#39;s test to highlight differences between and among groups.</li>
	<li>Perform statistical analysis using the statistical software program and consider a probability of P &#60; 0.05 to be the minimum level of significance. All results are expressed as mean &#177; S.E.M.</li>
</ol>

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G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Differences+in+the+kinetic+of+the+first+meiotic+division+and+in+active+mitochondrial+distribution+between+prepubertal+and+adult+oocytes+mirror+differences+in+their+developmental+competence+in+a+sheep+model.">Differences in the kinetic of the first meiotic division and in active mitochondrial distribution between prepubertal and adult oocytes mirror differences in their developmental competence in a sheep model.</a> PLoS ONE. 10 (4), (2015).</li><li>Berlinguer, F., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Effects+of+trehalose+co-incubation+on+in+vitro+matured+prepubertal+ovine+oocyte+vitrification.">Effects of trehalose co-incubation on in vitro matured prepubertal ovine oocyte vitrification.</a> Cryobiology. 55 (1), 27-34 (2007).</li><li>Serra, E., Gadau, S. D., Berlinguer, F., Naitana, S., Succu, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Morphological+features+and+microtubular+changes+in+vitrified+ovine+oocytes.">Morphological features and microtubular changes in vitrified ovine oocytes.</a> Theriogenology. 148, 216-224 (2020).</li><li>Asgari, V., Hosseini, S. M., Ostadhosseini, S., Hajian, M., Nasr-Esfahani, M. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Time+dependent+effect+of+post+warming+interval+on+microtubule+organization,+meiotic+status,+and+parthenogenetic+activation+of+vitrified+in+vitro+matured+sheep+oocytes.">Time dependent effect of post warming interval on microtubule organization, meiotic status, and parthenogenetic activation of vitrified in vitro matured sheep oocytes.</a> Theriogenology. 75 (5), 904-910 (2011).</li><li>Ciotti, P. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Meiotic+spindle+recovery+is+faster+in+vitrification+of+human+oocytes+compared+to+slow+freezing.">Meiotic spindle recovery is faster in vitrification of human oocytes compared to slow freezing.</a> Fertility and Sterility. 91 (6), 2399-2407 (2009).</li><li>Ledda, S., Bogliolo, L., Leoni, G., Naitana, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cell+Coupling+and+Maturation-Promoting+Factor+Activity+in+In+Vitro-Matured+Prepubertal+and+Adult+Sheep+Oocytes1.">Cell Coupling and Maturation-Promoting Factor Activity in In Vitro-Matured Prepubertal and Adult Sheep Oocytes1.</a> Biology of Reproduction. 65 (1), 247-252 (2001).</li><li>Palmerini, M. G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=In+vitro+maturation+is+slowed+in+prepubertal+lamb+oocytes:+ultrastructural+evidences.">In vitro maturation is slowed in prepubertal lamb oocytes: ultrastructural evidences.</a> Reproductive Biology and Endocrinology. 12, (2014).</li><li>Leoni, G. G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Relations+between+relative+mRNA+abundance+and+developmental+competence+of+ovine+oocytes.">Relations between relative mRNA abundance and developmental competence of ovine oocytes.</a> Molecular Reproduction and Development. 74 (2), 249-257 (2007).</li><li>Succu, S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Effect+of+vitrification+solutions+and+cooling+upon+in+vitro+matured+prepubertal+ovine+oocytes.">Effect of vitrification solutions and cooling upon in vitro matured prepubertal ovine oocytes.</a> Theriogenology. 68 (1), 107-114 (2007).</li><li>Larman, M. G., Sheehan, C. B., Gardner, D. K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Calcium-free+vitrification+reduces+cryoprotectant-induced+zona+pellucida+hardening+and+increases+fertilization+rates+in+mouse+oocytes.">Calcium-free vitrification reduces cryoprotectant-induced zona pellucida hardening and increases fertilization rates in mouse oocytes.</a> Reproduction. 131 (1), 53-61 (2006).</li><li>Yeste, M., Jones, C., Amdani, S. N., Patel, S., Coward, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Oocyte+activation+deficiency:+a+role+for+an+oocyte+contribution.">Oocyte activation deficiency: a role for an oocyte contribution.</a> Human Reproduction Update. 22 (1), 23-47 (2016).</li><li>Rienzi, L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Oocyte,+embryo+and+blastocyst+cryopreservation+in+ART:+systematic+review+and+meta-analysis+comparing+slow-freezing+versus+vitrification+to+produce+evidence+for+the+development+of+global+guidance.">Oocyte, embryo and blastocyst cryopreservation in ART: systematic review and meta-analysis comparing slow-freezing versus vitrification to produce evidence for the development of global guidance.</a> Human Reproduction Update. 23 (2), 139-155 (2017).</li><li>De Santis, L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Oocyte+vitrification:+influence+of+operator+and+learning+time+on+survival+and+development+parameters.">Oocyte vitrification: influence of operator and learning time on survival and development parameters.</a> Placenta. 32, 280-281 (2011).</li><li>Zhang, X., Catalano, P. N., Gurkan, U. A., Khimji, I., Demirci, U. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Emerging+technologies+in+medical+applications+of+minimum+volume+vitrification.">Emerging technologies in medical applications of minimum volume vitrification.</a> Nanomedicine. 6 (6), 1115-1129 (2011).</li></ol>

The authors declare they have no competing financial interests.

Oocyte cryopreservation in domestic animals can allow not only the long-term conservation of female genetic resources, but also advance the development of embryonic biotechnologies. Thus, the development of a standard method for oocyte vitrification would advantage both the livestock and the research sector. In this protocol, a complete method for adult sheep oocyte vitrification is presented and could represent a solid starting point for the development of an efficient vitrification system for juvenile oocyte.
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Long-term storage of the female gametes can offer a wide range of applications, such as improving domestic animal breeding by genetic selection programs, contributing to preserve biodiversity through the ex-situ wildlife species conservation program, and boosting in vitro biotechnology research and applications thanks to the availability of stored oocytes to be incorporated in in vitro embryo production or nuclear transplantation programs1,2,3. Juvenile oocyte vitrification would also increase genetic gain by shortening the generation interval in breeding programs4. Vitrification by ultra-rapid cooling and warming of oocytes is currently considered a standard approach for livestock oocytes cryopreservation5. In ruminants, before vitrification, oocytes are usually matured in vitro, after retrieval from follicles obtained from abattoir-derived ovaries2. Adult, and especially prepubertal ovaries4,6, can indeed supply a virtually unlimited number of oocytes to be cryopreserved.
In cattle, after oocyte vitrification and warming, blastocyst yields at &#62;10% have been commonly reported by several laboratories during the last decade3. However, in small ruminants oocyte vitrification is still considered relatively new for both juvenile and adult oocytes, and a standard method for sheep oocyte vitrification remains to be established2,5. Despite recent advancements, the vitrified and warmed oocyte indeed presents several functional and structural alterations that limit their developmental potential7,8,9. Thus, few articles have reported blastocyst development at 10% or more in vitrified/warmed sheep oocytes2. Several approaches have been investigated to reduce the above-mentioned alterations: optimizing the composition of the vitrification and thawing solutions10,11; experimenting with the use of different cryo-devices8,12,13; and applying specific treatments during in vitro maturation (IVM)4,14,15 and/or during the recovery time after warming6.
Here we describe a protocol for the vitrification of sheep oocytes collected from juvenile and adult donors and matured in vitro prior to cryopreservation. The protocol includes all the procedures from oocyte in vitro maturation to vitrification, warming and post-warming culture period.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>2&#8242;,7&#8242;-Dichlorofluorescin diacetate</td>
			<td>Sigma-Aldrich</td>
			<td>D-6883</td>
			<td></td>
		</tr>
		<tr>
			<td>Albumin bovine fraction V, protease free</td>
			<td>Sigma-Aldrich</td>
			<td>A3059</td>
			<td></td>
		</tr>
		<tr>
			<td>Bisbenzimide H 33342 trihydrochloride (Hoechst 33342)</td>
			<td>Sigma-Aldrich</td>
			<td>14533</td>
			<td></td>
		</tr>
		<tr>
			<td>Calcium chloride (CaCl2 2H20)</td>
			<td>Sigma-Aldrich</td>
			<td>C8106</td>
			<td></td>
		</tr>
		<tr>
			<td>Citric acid</td>
			<td>Sigma-Aldrich</td>
			<td>C2404</td>
			<td></td>
		</tr>
		<tr>
			<td>Confocal laser scanning microscope</td>
			<td>Leica Microsystems GmbH,Wetzlar</td>
			<td>TCS SP5 DMI 6000CS</td>
			<td></td>
		</tr>
		<tr>
			<td>Cryotop Kitazato</td>
			<td>Medical Biological Technologies</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Cysteamine</td>
			<td>Sigma-Aldrich</td>
			<td>M9768</td>
			<td></td>
		</tr>
		<tr>
			<td>D- (-) Fructose</td>
			<td>Sigma-Aldrich</td>
			<td>F0127</td>
			<td></td>
		</tr>
		<tr>
			<td>D(+)Trehalose dehydrate</td>
			<td>Sigma-Aldrich</td>
			<td>T0167</td>
			<td></td>
		</tr>
		<tr>
			<td>Dimethyl sulfoxide (DMSO)</td>
			<td>Sigma-Aldrich</td>
			<td>D2438</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco Phosphate Buffered Saline</td>
			<td>Sigma-Aldrich</td>
			<td>D8537</td>
			<td></td>
		</tr>
		<tr>
			<td>Egg yolk</td>
			<td>Sigma-Aldrich</td>
			<td>P3556</td>
			<td></td>
		</tr>
		<tr>
			<td>Ethylene glycol (EG)</td>
			<td>Sigma-Aldrich</td>
			<td>324558</td>
			<td></td>
		</tr>
		<tr>
			<td>FSH</td>
			<td>Sigma-Aldrich</td>
			<td>F4021</td>
			<td></td>
		</tr>
		<tr>
			<td>Glutamic Acid</td>
			<td>Sigma-Aldrich</td>
			<td>G5638</td>
			<td></td>
		</tr>
		<tr>
			<td>Glutaraldehyde</td>
			<td>Sigma-Aldrich</td>
			<td>G5882</td>
			<td></td>
		</tr>
		<tr>
			<td>Glycerol</td>
			<td>Sigma-Aldrich</td>
			<td>G5516</td>
			<td></td>
		</tr>
		<tr>
			<td>Glycine</td>
			<td>Sigma-Aldrich</td>
			<td>G8790</td>
			<td></td>
		</tr>
		<tr>
			<td>Heparin</td>
			<td>Sigma-Aldrich</td>
			<td>H4149</td>
			<td></td>
		</tr>
		<tr>
			<td>HEPES</td>
			<td>Sigma-Aldrich</td>
			<td>H4034</td>
			<td></td>
		</tr>
		<tr>
			<td>Hypoutarine</td>
			<td>Sigma-Aldrich</td>
			<td>H1384</td>
			<td></td>
		</tr>
		<tr>
			<td>Inverted microscope</td>
			<td>Diaphot, Nikon</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>L-Alanine</td>
			<td>Sigma-Aldrich</td>
			<td>A3534</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Arginine</td>
			<td>Sigma-Aldrich</td>
			<td>A3784</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Asparagine</td>
			<td>Sigma-Aldrich</td>
			<td>A4284</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Aspartic Acid</td>
			<td>Sigma-Aldrich</td>
			<td>A4534</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Cysteine</td>
			<td>Sigma-Aldrich</td>
			<td>C7352</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Cystine</td>
			<td>Sigma-Aldrich</td>
			<td>C8786</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Glutamine</td>
			<td>Sigma-Aldrich</td>
			<td>G3126</td>
			<td></td>
		</tr>
		<tr>
			<td>LH</td>
			<td>Sigma-Aldrich</td>
			<td>L6420</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Histidine</td>
			<td>Sigma-Aldrich</td>
			<td>H9511</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Isoleucine</td>
			<td>Sigma-Aldrich</td>
			<td>I7383</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Leucine</td>
			<td>Sigma-Aldrich</td>
			<td>L1512</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Lysine</td>
			<td>Sigma-Aldrich</td>
			<td>L1137</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Methionine</td>
			<td>Sigma-Aldrich</td>
			<td>M2893</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Ornithine</td>
			<td>Sigma-Aldrich</td>
			<td>O6503</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Phenylalanine</td>
			<td>Sigma-Aldrich</td>
			<td>P5030</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Proline</td>
			<td>Sigma-Aldrich</td>
			<td>P4655</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Serine</td>
			<td>Sigma-Aldrich</td>
			<td>S5511</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Tyrosine</td>
			<td>Sigma-Aldrich</td>
			<td>T1020</td>
			<td></td>
		</tr>
		<tr>
			<td>L-Valine</td>
			<td>Sigma-Aldrich</td>
			<td>V6504</td>
			<td></td>
		</tr>
		<tr>
			<td>Magnesium chloride heptahydrate (MgSO4.7H2O)</td>
			<td>Sigma-Aldrich</td>
			<td>M2393</td>
			<td></td>
		</tr>
		<tr>
			<td>Makler Counting Chamber</td>
			<td>Sefi-Medical Instruments ltd.Biosigma S.r.l.</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Medium 199</td>
			<td>Sigma-Aldrich</td>
			<td>M5017</td>
			<td></td>
		</tr>
		<tr>
			<td>Mineral oil</td>
			<td>Sigma-Aldrich</td>
			<td>M8410</td>
			<td></td>
		</tr>
		<tr>
			<td>MitoTracker Red CM-H2XRos</td>
			<td>ThermoFisher</td>
			<td>M7512</td>
			<td></td>
		</tr>
		<tr>
			<td>New born calf serum heat inactivated (FCS)</td>
			<td>Sigma-Aldrich</td>
			<td>N4762</td>
			<td></td>
		</tr>
		<tr>
			<td>Penicillin G sodium salt</td>
			<td>Sigma-Aldrich</td>
			<td>P3032</td>
			<td></td>
		</tr>
		<tr>
			<td>Phenol Red</td>
			<td>Sigma-Aldrich</td>
			<td>P3532</td>
			<td></td>
		</tr>
		<tr>
			<td>Polyvinyl alcohol (87-90% hydrolyzed, average mol wt 30,000-70,000)</td>
			<td>Sigma-Aldrich</td>
			<td>P8136</td>
			<td></td>
		</tr>
		<tr>
			<td>Potassium Chloride (KCl)</td>
			<td>Sigma-Aldrich</td>
			<td>P5405</td>
			<td></td>
		</tr>
		<tr>
			<td>Potassium phosphate monobasic (KH2PO4)</td>
			<td>Sigma-Aldrich</td>
			<td>P5655</td>
			<td></td>
		</tr>
		<tr>
			<td>Propidium iodide</td>
			<td>Sigma-Aldrich</td>
			<td>P4170</td>
			<td></td>
		</tr>
		<tr>
			<td>Sheep serum</td>
			<td>Sigma-Aldrich</td>
			<td>S2263</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium azide</td>
			<td>Sigma-Aldrich</td>
			<td>S2202</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium bicarbonate (NaHCO3)</td>
			<td>Sigma-Aldrich</td>
			<td>S5761</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium chloride (NaCl)</td>
			<td>Sigma-Aldrich</td>
			<td>S9888</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium dl-lactate solution syrup</td>
			<td>Sigma-Aldrich</td>
			<td>L4263</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium pyruvate</td>
			<td>Sigma-Aldrich</td>
			<td>P2256</td>
			<td></td>
		</tr>
		<tr>
			<td>Sperm Class Analyzer</td>
			<td>Microptic S.L.</td>
			<td>S.C.A. v 3.2.0</td>
			<td></td>
		</tr>
		<tr>
			<td>Statistical software Minitab 18.1</td>
			<td>2017 Minitab</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Stereo microscope</td>
			<td>Olimpus</td>
			<td>SZ61</td>
			<td></td>
		</tr>
		<tr>
			<td>Streptomycin sulfate</td>
			<td>Sigma-Aldrich</td>
			<td>S9137</td>
			<td></td>
		</tr>
		<tr>
			<td>Taurine</td>
			<td>Sigma-Aldrich</td>
			<td>T7146</td>
			<td></td>
		</tr>
		<tr>
			<td>TRIS</td>
			<td>Sigma-Aldrich</td>
			<td>15,456-3</td>
			<td></td>
		</tr>
	</tbody>
</table>

vitrification of in vitro matured oocytes collected from adult and prepubertal ovaries in sheep

In livestock, in vitro embryo production systems can be developed and sustained thanks to the large number of ovaries and oocytes that can be easily obtained from a slaughterhouse. Adult ovaries always bear several antral follicles, while in pre-pubertal donors the maximal numbers of oocytes are available at 4 weeks of age, when ovaries bear peak numbers of antral follicles. Thus, 4 weeks old lambs are considered good donors, even if the developmental competence of prepubertal oocytes is lower compared to their adult counterpart. 
Basic research and commercial applications would be boosted by the possibility of successfully cryopreserving vitrified oocytes obtained from both adult and prepubertal donors. The vitrification of oocyte collected from prepubertal donors would also allow shortening the generation interval and thus increasing the genetic gain in breeding programs. However, the loss of developmental potential after cryopreservation makes mammalian oocytes probably one of the most difficult cell types to cryopreserve. Among the available cryopreservation techniques, vitrification is widely applied to animal and human oocytes. Despite recent advancements in the technique, exposures to high concentrations of cryoprotective agents as well as chilling injury and osmotic stress still induce several structural and molecular alterations and reduce the developmental potential of mammalian oocytes. Here, we describe a protocol for the vitrification of sheep oocytes collected from juvenile and adult donors and matured in vitro prior to cryopreservation. The protocol includes all the procedures from oocyte in vitro maturation to vitrification, warming and post-warming incubation period. Oocytes vitrified at the MII stage can indeed be fertilized following warming, but they need extra time prior to fertilization to restore damage due to cryopreservation procedures and to increase their developmental potential. Thus, post-warming culture conditions and timing are crucial steps for the restoration of oocyte developmental potential, especially when oocyte are collected from juvenile donors.

The cryotolerance of oocyte from juvenile donors is lower compared to adult ones. The first effect observed is a lower post-warming survival rate compared to adult oocytes (Figure 1A; &#967;2 test P&#60;0.001). Juvenile oocytes showed a lower membrane integrity after warming (Figure 1B). The use of trehalose in the maturation medium was intended to verify whether this sugar could reduce cryoinjuries in juvenile oocytes. The data have demonstrated<sup ...

Watch this Scientific Journal Video about Vitrification of In Vitro Matured Oocytes Collected from Adult and Prepubertal Ovaries in Sheep at JoVE.com

Vitrification of In Vitro Matured Oocytes Collected from Adult and Prepubertal Ovaries in Sheep

The protocol aims at providing a standard method for the vitrification of adult and juvenile sheep oocytes. It includes all the steps from the preparation of the in vitro maturation media to the post-warming culture. Oocytes are vitrified at the MII stage using Cryotop to ensure the minimum essential volume.

In livestock, in vitro embryo production systems can be developed and sustained thanks to the large number of ovaries and oocytes that can be easily ...

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Developmental Biology

5.0K Views.  University of Sassari. The protocol aims at providing a standard method for the vitrification of adult and juvenile sheep oocytes. It includes all the steps from the preparation of the in vitro maturation media to the post-warming culture. Oocytes are vitrified at the MII stage using Cryotop to ensure the minimum essential volume. 

Video: Vitrification of In Vitro Matured Oocytes Collected from Adult and Prepubertal Ovaries in Sheep

Manipulation and In Vitro Maturation of Xenopus laevis Oocytes, Followed by Intracytoplasmic Sperm Injection, to Study Embryonic Development

Amphibian eggs have been widely used to study embryonic development. Early embryonic development is driven by maternally stored factors accumulated during oogenesis. In order to study roles of such maternal factors in early embryonic development, it is desirable to manipulate their functions from the very beginning of embryonic development. Conventional ways of gene interference are achieved by injection of antisense oligonucleotides (oligos) or mRNA into fertilized eggs, enabling under- or over-expression of specific proteins, respectively. However, these methods normally require more than several hours until protein expression is affected, and, hence, the interference of gene functions is not effective during early embryonic stages. Here, we introduce an experimental system in which expression levels of maternal proteins can be altered before fertilization. Xenopus laevis oocytes obtained from ovaries are defolliculated by incubating with enzymes. Antisense oligos or mRNAs are injected into defolliculated oocytes at the germinal vesicle (GV) stage. These oocytes are in vitro matured to eggs at the metaphase II (MII) stage, followed by intracytoplasmic sperm injection (ICSI). By this way, up to 10% of ICSI embryos can reach the swimming tadpole stage, thus allowing functional tests of specific gene knockdown or overexpression. This approach can be a useful way to study roles of maternally stored factors in early embryonic development.

Manipulation and In Vitro Maturation of Xenopus laevis Oocytes, Followed by Intracytoplasmic Sperm Injection, to Study Embryonic Development

We describe methods of manipulating Xenopus laevis immature oocytes, in vitro maturation of oocytes to eggs, and intracytoplasmic sperm injection. This protocol allows degradation of some maternal proteins and overexpression of genes of interest at fertilization, and hence is valuable to study roles of specific factors in early embryonic development.

Amphibian eggs have been widely used to study embryonic development. Early embryonic development is driven by maternally stored factors accumulated during ...

In Vitro Colony Assays for Characterizing Tri-potent Progenitor Cells Isolated from the Adult Murine Pancreas

Stem and progenitor cells from the adult pancreas could be a potential source of therapeutic beta-like cells for treating patients with type 1 diabetes. However, it is still unknown whether stem and progenitor cells exist in the adult pancreas. Research strategies using cre-lox lineage-tracing in adult mice have yielded results that either support or refute the idea that beta cells can be generated from the ducts, the presumed location where adult pancreatic progenitors may reside. These in vivo cre-lox lineage-tracing methods, however, cannot answer the questions of self-renewal and multi-lineage differentiation-two criteria necessary to define a stem cell. To begin addressing this technical gap, we devised 3-dimensional colony assays for pancreatic progenitors. Soon after our initial publication, other laboratories independently developed a similar, but not identical, method called the organoid assay. Compared to the organoid assay, our method employs methylcellulose, which forms viscous solutions that allow the inclusion of extracellular matrix proteins at low concentrations. The methylcellulose-containing assays permit easier detection and analyses of progenitor cells at the single-cell level, which are critical when progenitors constitute a small sub-population, as is the case for many adult organ stem cells. Together, results from several laboratories demonstrate in vitro self-renewal and multi-lineage differentiation of pancreatic progenitor-like cells from mice. The current protocols describe two methylcellulose-based colony assays to characterize mouse pancreatic progenitors; one contains a commercial preparation of murine extracellular matrix proteins and the other an artificial extracellular matrix protein known as a laminin hydrogel. The techniques shown here are 1) dissociation of the pancreas and sorting of CD133+Sox9/EGFP+ ductal cells from adult mice, 2) single cell manipulation of the sorted cells, 3) single colony analyses using microfluidic qRT-PCR and whole-mount immunostaining, and 4) dissociation of primary colonies into single-cell suspensions and re-plating into secondary colony assays to assess self-renewal or differentiation.

In Vitro Colony Assays for Characterizing Tri-potent Progenitor Cells Isolated from the Adult Murine Pancreas

In vitro colony assays to detect self-renewal and differentiation of progenitor cells isolated from adult murine pancreas are devised. In these assays, pancreatic progenitors give rise to cell colonies in 3-dimensional space in methylcellulose-containing semi-solid medium. Protocols for handling single cells and characterization of individual colonies are described.

Stem and progenitor cells from the adult pancreas could be a potential source of therapeutic beta-like cells for treating patients with type 1 diabetes. ...

Directed Differentiation of Primitive and Definitive Hematopoietic Progenitors from Human Pluripotent Stem Cells

One of the major goals for regenerative medicine is the generation and maintenance of hematopoietic stem cells (HSCs) derived from human pluripotent stem cells (hPSCs). Until recently, efforts to differentiate hPSCs into HSCs have predominantly generated hematopoietic progenitors that lack HSC potential, and instead resemble yolk sac hematopoiesis.&#160;These resulting hematopoietic progenitors may have limited utility for in vitro disease modeling of various adult hematopoietic disorders, particularly those of the lymphoid lineages. However, we have recently described methods to generate erythro-myelo-lymphoid multilineage definitive hematopoietic progenitors from hPSCs using a stage-specific directed differentiation protocol, which we outline here. Through enzymatic dissociation of hPSCs on basement membrane matrix-coated plasticware, embryoid bodies (EBs) are formed. EBs are differentiated to mesoderm by recombinant BMP4, which is subsequently specified to the definitive hematopoietic program by the GSK3&#946; inhibitor, CHIR99021. Alternatively, primitive hematopoiesis is specified by the PORCN inhibitor, IWP2. Hematopoiesis is further driven through the addition of recombinant VEGF and supportive hematopoietic cytokines. The resulting hematopoietic progenitors generated using this method have the potential to be used for disease and developmental modeling, in vitro.

Here, we present human pluripotent stem cell (hPSC) culture protocols, used to differentiate hPSCs into CD34+ hematopoietic progenitors. This method uses stage-specific manipulation of canonical WNT signaling to specify cells exclusively to either the definitive or primitive hematopoietic program.

One of the major goals for regenerative medicine is the generation and maintenance of hematopoietic stem cells (HSCs) derived from human pluripotent stem ...

Dissection and Immunofluorescent Staining of Mushroom Body and Photoreceptor Neurons in Adult Drosophila melanogaster Brains

Nervous system development involves a sequential series of events that are coordinated by several signaling pathways and regulatory networks. Many of the proteins involved in these pathways are evolutionarily conserved between mammals and other eukaryotes, such as the fruit fly Drosophila melanogaster, suggesting that similar organizing principles exist during the development of these organisms. Importantly, Drosophila has been used extensively to identify cellular and molecular mechanisms regulating processes that are required in mammals including neurogenesis, differentiation, axonal guidance, and synaptogenesis. Flies have also been used successfully to model a variety of human neurodevelopmental diseases. Here we describe a protocol for the step-by-step microdissection, fixation, and immunofluorescent localization of proteins within the adult Drosophila brain. This protocol focuses on two example neuronal populations, mushroom body neurons and retinal photoreceptors, and includes optional steps to trace individual mushroom body neurons using Mosaic Analysis with a Repressible Cell Marker (MARCM) technique. Example data from both wild-type and mutant brains are shown along with a brief description of a scoring criteria for axonal guidance defects. While this protocol highlights two well-established antibodies for investigating the morphology of mushroom body and photoreceptor neurons, other Drosophila brain regions and the localization of proteins within other brain regions can also be investigated using this protocol.

Dissection and Immunofluorescent Staining of Mushroom Body and Photoreceptor Neurons in Adult Drosophila melanogaster Brains

This protocol describes the dissection and immunostaining of adult Drosophila melanogaster brain tissues. Specifically, this protocol highlights the use of Drosophila mushroom body and photoreceptor neurons as example neuronal subsets that can be accurately used to uncover general principles underlying many aspects of neuronal development.

Nervous system development involves a sequential series of events that are coordinated by several signaling pathways and regulatory networks. Many of the ...

Dissection and Staining of Drosophila Pupal Ovaries

Unlike adult Drosophila ovaries, pupal ovaries are relatively difficult to access and examine due to their small size, translucence, and encasing within a pupal case. The challenge of dissecting pupal ovaries also lies in their physical location within the pupa: the ovaries are surrounded by fat body cells inside the pupal abdomen, and these fat cells must be removed to allow for proper antibody staining. To overcome these challenges, this protocol utilizes customized Pasteur pipets to extract fat body cells from the pupal abdomen. Moreover, a chambered coverglass is used in place of a microcentrifuge tube during the staining process to improve visibility of the pupae. However, despite these and other advantages of the tools used in this protocol, successful execution of these techniques may still involve several days of practice due to the small size of pupal ovaries. The techniques outlined in this protocol could be applied to time course experiments in which ovaries are analyzed at various stages of pupal development.

Dissection and Staining of Drosophila Pupal Ovaries

The Drosophila ovary is an excellent model system for studying stem cell niche development. Though methods for dissecting larval and adult ovaries have been published, pupal ovary dissections require different techniques that have not been published in detail. Here we outline a protocol for dissecting, staining, and mounting pupal ovaries.

Unlike adult Drosophila ovaries, pupal ovaries are relatively difficult to access and examine due to their small size, translucence, and encasing within a ...

Generation of Scaffold-free, Three-dimensional Insulin Expressing Pancreatoids from Mouse Pancreatic Progenitors In Vitro

The pancreas is a complex organ composed of many different cell types that work together to regulate blood glucose homeostasis and digestion. These cell types include enzyme-secreting acinar cells, an arborized ductal system responsible for the transportation of enzymes to the gut, and hormone-producing endocrine cells. 
Endocrine beta-cells are the sole cell type in the body that produce insulin to lower blood glucose levels. Diabetes, a disease characterized by a loss or the dysfunction of beta-cells, is reaching epidemic proportions. Thus, it is essential to establish protocols to investigate beta-cell development that can be used for screening purposes to derive the drug and cell-based therapeutics. While the experimental investigation of mouse development is essential, in vivo studies are laborious and time-consuming. Cultured cells provide a more convenient platform for screening; however, they are unable to maintain the cellular diversity, architectural organization, and cellular interactions found in vivo. Thus, it is essential to develop new tools to investigate pancreatic organogenesis and physiology.
Pancreatic epithelial cells develop in the close association with mesenchyme from the onset of organogenesis as cells organize and differentiate into the complex, physiologically competent adult organ. The pancreatic mesenchyme provides important signals for the endocrine development, many of which are not well understood yet, thus difficult to recapitulate during the in vitro culture. Here, we describe a protocol to culture three-dimensional, cellular complex mouse organoids that retain mesenchyme, termed pancreatoids. The e10.5 murine pancreatic bud is dissected, dissociated, and cultured in a scaffold-free environment. These floating cells self-assemble with mesenchyme enveloping the developing pancreatoid and a robust number of endocrine beta-cells developing along with the acinar and the duct cells. This system can be used to study the cell fate determination, structural organization, and morphogenesis, cell-cell interactions during organogenesis, or for the drug, small molecule, or genetic screening.

Generation of Scaffold-free, Three-dimensional Insulin Expressing Pancreatoids from Mouse Pancreatic Progenitors In Vitro

Here, we present a protocol to generate insulin expressing 3D murine pancreatoids from free-floating e10.5 dissociated pancreatic progenitors and the associated mesenchyme.

The pancreas is a complex organ composed of many different cell types that work together to regulate blood glucose homeostasis and digestion. These cell ...

Human Blastocyst Biopsy and Vitrification

Blastocyst biopsy is performed to obtain a reliable genetic diagnosis during IVF cycles with preimplantation genetic testing. Then, the ideal workflow entails a safe and efficient vitrification protocol, due to the turnaround time of the diagnostic techniques and to transfer the selected embryo(s) on a physiological endometrium in a following natural cycle. A biopsy approach encompassing the sequential opening of the zona pellucida and retrieval of 5-10 trophectoderm cells (ideally 7-8) limits both the number of manipulations required and the exposure of the embryo to sub-optimal environmental conditions. After proper training, the technique was reproducible across different operators in terms of timing of biopsy (~8 min, ranging 3-22 min based on the number of embryos to biopsy per dish), conclusive diagnoses obtained (~97.5%) and live birth rates after vitrified-warmed euploid blastocyst transfer (&#62;40%). The survival rate after biopsy, vitrification and warming was as high as 99.8%. The re-expansion rate at 1.5 h from warming was as high as 97%, largely dependent on the timing between biopsy and vitrification (ideally &#8804;30 min), blastocyst morphological quality and day of biopsy. In general, it is better to vitrify a collapsed blastocyst; therefore, in non-PGT cycles, laser-assisted artificial shrinkage might be performed to induce embryo collapse prior to cryopreservation. The most promising future perspective is the non-invasive analysis of the IVF culture media after blastocyst culture as a putative source of embryonic DNA. However, this potential avant-garde is still under investigation and a reliable protocol yet needs to be defined and validated.

Blastocyst biopsy and vitrification are required to efficiently conduct preimplantation genetic testing. An approach entailing the sequential opening of the zona pellucida and retrieval of 7-8 trophectoderm cells in day 5-7 post-insemination limits both the number of manipulations required and the exposure of the embryo to sub-optimal environmental conditions.

Blastocyst biopsy is performed to obtain a reliable genetic diagnosis during IVF cycles with preimplantation genetic testing. Then, the ideal workflow ...

Minimum Volume Vitrification of Immature Feline Oocytes

In wild animals&#8217; conservation programs, gamete banking is crucial to safeguard genetic resources of valuable individuals and rare species and to promote biodiversity preservation. In felids, most species are threatened with extinction, and domestic breeds are used as a model to increase the efficiency of protocols for germplasm banking. Among oocyte cryopreservation techniques, vitrification is more and more popular in human and veterinary assisted reproduction. Cryotop vitrification, which was at first developed for human oocytes and embryos, has demonstrated to be well-suited for cat oocytes. This method offers several advantages, such as the feasibility in field conditions and the speed of the procedure, which can be helpful when several samples need to be processed. However, the efficiency is strongly dependent on the operator&#8217;s skills, and intra- and inter-laboratory standardization are needed, as well as personnel training. This protocol describes minimum volume vitrification of immature feline oocytes on a commercial support in a step by step field-friendly protocol, from oocyte collection to warming. Following the protocol, preservation of oocyte integrity and viability at warming (as high as 90%) can be expected, although there is still room for improvement in post-warming maturation and embryonic development outcomes.

This manuscript describes a protocol for the minimum volume vitrification of immature cat oocytes with laboratory-made media on commercial supports. It covers every step from oocyte isolation from ex vivo gonads to vitrification and warming.

In wild animals&#8217; conservation programs, gamete banking is crucial to safeguard genetic resources of valuable individuals and rare species and to ...

In Vitro Culture Strategy for Oocytes from Early Antral Follicle in Cattle

The limited reserve of mature, fertilizable oocytes represents a major barrier for the success of assisted reproduction in mammals. Considering that during the reproductive life span only about 1% of the oocytes in an ovary mature and ovulate, several techniques have been developed to increase the exploitation of the ovarian reserve to the growing population of non-ovulatory follicles. Such technologies have allowed interventions of fertility preservation, selection programs in livestock, and conservation of endangered species. However, the vast potential of the ovarian reserve is still largely unexploited. In cows, for instance, some attempts have been made to support in vitro culture of oocytes at specific developmental stages, but efficient and reliable protocols have not yet been developed. Here we describe a culture system that reproduce the physiological conditions of the corresponding follicular stage, defined to develop in vitro growing oocytes collected from bovine early antral follicles to the fully-grown stage, corresponding to the medium antral follicle in vivo. A combination of hormones and a phosphodiesterase 3 inhibitor was used to prevent untimely meiotic resumption and to guide oocyte&#39;s differentiation.

We describe the procedures for isolation of growing oocytes from ovarian follicles at early stages of development, as well as the setup of an in vitro culture system which can support the growth and differentiation up to the fully-grown stage. &#160;

The limited reserve of mature, fertilizable oocytes represents a major barrier for the success of assisted reproduction in mammals. Considering that ...

Accurate Follicle Enumeration in Adult Mouse Ovaries

Sexually reproducing female mammals are born with their entire lifetime supply of oocytes. Immature, quiescent oocytes are found within primordial follicles, the storage unit of the female germline. They are non-renewable, thus their number at birth and subsequent rate of loss largely dictates the female fertile lifespan. Accurate quantification of primordial follicle numbers in women and animals is essential for determining the impact of medicines and toxicants on the ovarian reserve. It is also necessary for evaluating the need for, and success of, existing and emerging fertility preservation techniques. Currently, no methods exist to accurately measure the number of primordial follicles comprising the ovarian reserve in women. Furthermore, obtaining ovarian tissue from large animals or endangered species for experimentation is often not feasible. Thus, mice have become an essential model for such studies, and the ability to evaluate primordial follicle numbers in whole mouse ovaries is a critical tool. However, reports of absolute follicle numbers in mouse ovaries in the literature are highly variable, making it difficult to compare and/or replicate data. This is due to a number of factors including strain, age, treatment groups, as well as technical differences in the methods of counting employed. In this article, we provide a step-by-step instructional guide for preparing histological sections and counting primordial follicles in mouse ovaries using two different methods: [1] stereology, which relies on the fractionator/optical dissector technique; and [2] the direct count technique. Some of the key advantages and drawbacks of each method will be highlighted so that reproducibility can be improved in the field and to enable researchers to select the most appropriate method for their studies.

Here, we describe, compare, and contrast two different techniques for accurate follicle counting of fixed mouse ovarian tissues.