Name: accurate follicle enumeration in adult mouse ovaries
Uploaded: 2020-10-16T15:00:00.000+00:00
Duration: 7 min 27 s
Description: Watch this Scientific Journal Video about Accurate Follicle Enumeration in Adult Mouse Ovaries at JoVE.com

This work was made possible through Victorian State Government Operational Infrastructure Support and Australian Government NHMRC IRIISS and supported by funding from National Health and Medical Research Council (ALW #1120300) and Australian Research Council (KJH #FT190100265). The authors would like to acknowledge the technical support of the Monash Animal Research Platform, Monash Histology Platform and Monash Micro Imaging facility.

Ovaries were collected from female C57BL6J mice. All animal procedures and experiments were performed in accordance with the NHMRC Australian Code of Practice for the Care and Use of Animals and approved by the Monash Animal Research Platform Animal Ethics Committee.
NOTE: A chemotherapy agent shown to deplete primordial follicle oocytes, as determined using stereology11 and direct counts12,13 was used in this report to compare the two counting methods in the same animal. Female, 8-week-old (young adult) mice were weighed prior to a single intraperitoneal injection of 75 mg/kg/bodyweight of cyclophosphamide, or saline vehicle control (n=5/group). This dose has been shown to cause an approximate 50% depletion of primordial follicles, but not reported to cause morbidity or mortality in mice14. Ovaries were harvested 48 hours after treatment. One ovary from each animal was fixed in 10% (v/v) neutral buffered formalin solution for 24 hours, and the other fixed in Bouin’s solution for 24 hours. Tissue was then embedded in either glycolmethacrylate resin and serially sectioned at 20 µm, or in paraffin and serially sectioned at 5 µm. All tissues were stained with periodic acid Schiff and haematoxylin.
1. Histological preparation: fixation, processing, embedding and sectioning mouse ovaries
<ol>
	<li>Dissect mouse ovaries by trimming the oviduct and all surrounding fat, without damaging or cutting the ovary itself. If necessary, use a dissecting microscope and fine blade for this step (Figure 1A).</li>
	<li>Fix tissues immediately by placing into a small labelled tube containing either Bouin’s fixative (stereology), or formalin fixative (direct counts) for 24 hours (Figure 1B), before transferring tissues into 70% ethanol. 
	NOTE: Follicle morphology is conserved best within Bouin’s fixed ovarian tissue, embedded into glycolmethacrylate resin (Figure 2).</li>
	<li>Process whole fixed ovaries and then embed in glycolmethacrylate resin for stereology (Supplementary File 1), or paraffin wax for direct counts using a standard histological protocol. 
	CAUTION: Resin is toxic, so ensure all tissue processing steps are performed in a fume hood and gloves are worn at all times.</li>
	<li>Use a specialized resin methacrylate microtome (Figure 1C) fitted with a glass knife (Figure 1D) to exhaustively cut thick glycolmethacrylate resin sections (e.g., 20 µm). Collect the sections at a regular interval (e.g., every 3rd section) onto glass microscope slides for stereology.</li>
	<li>Use a standard microtome to cut thin paraffin sections (e.g., 4-6 µm). Collect tissue sections at a regular interval (e.g., every 9th section) onto a glass microscope slide for direct follicle counts.</li>
	<li>Stain the slides with periodic acid Schiff and haematoxylin (Supplementary File 2).</li>
	<li>Coverslip with standard DPX for paraffin sections, or thick DPX for glycolmethacrylate resin sections (Figure 1E). 
	CAUTION: Glycolmethacrylate resin DPX is hazardous, so perform this step in to fume hood. 
	NOTE: Glycolmethacrylate resin DPX is extremely viscous. The glass coverslip must be adhered firmly by pressing it down with a spatula to ensure the DPX is evenly and thinly dispersed, and there are no air bubbles present under the coverslip (Figure 1F).</li>
</ol>
2. Stereological estimation of primordial follicle number using the optical fractionator
<ol>
	<li>Turn on the computer, the multi-control unit, the camera and the light source within the stereology setup and set the microscope objective to a low magnification (e.g., 10x).</li>
	<li>Open the stereology software.</li>
	<li>Put the first slide securely on the microscope stage.</li>
	<li>Adjust the light exposure by checking Automatic under Exposure in the Camera Settings panel (Supplementary Figure 1A). Alternatively, manually adjust the light exposure.</li>
	<li>Use the joystick to locate the first tissue sample and bring the sample into focus.</li>
	<li>Adjust the white balance, either by clicking on More Settings (located bottom right of the Camera Settings panel), and then click White Balance and click on Automatic (Supplementary Figure 1B). Alternatively, click the White Balance button adjacent to the More Settings button (or Select Area in More Settings), to set the white balance manually by selecting a white area on the section.</li>
	<li>Go to the Probes drop down menu and click on Optical Fractionator Workflow. Then click Start New Project and click OK.
	<ol>
		<li>If an existing sampling configuration has been saved, under Sampling Parameters click Yes | … and select the desired sampling configuration.</li>
		<li>If not, click No and manually enter the serial section information (Supplementary Figure 1C) and define the probe configuration at step 2.13.</li>
	</ol>
	</li>
	<li>Click on Next, set the microscope to Low Magnification and choose 10x magnification from the dropdown menu.</li>
	<li>Click on Next, and then trace around the entire ovarian section – start by left clicking around the section and at the end, right click and choose Close Contour.</li>
	<li>Click on Next, set the microscope to High Magnification and choose 100x Oil magnification from the dropdown menu.</li>
	<li>Place a drop of oil on the tissue section on the slide and move the microscope objective to 100x magnification.</li>
	<li>Adjust the light exposure (as in step 2.4) and click Next.</li>
	<li>Set up the Sampling Parameters to define the probe configuration. Here, the counting frame was set to 47.5 µm x 47.5 µm (2,256.25 µm2) and the step length was set to 100 µm x 100 µm (10,000 µm2) (Supplementary Figure 2). Once the sampling parameters are established, save the template and re-open during subsequent analysis sessions at step 2.7.</li>
	<li>Click on Start Counting (Supplementary Figure 1D). Focus to the top of the sample, click OK and begin counting.</li>
	<li>Use the focusing knob to move through the 10 µm sampling depth and count any primordial follicles whose oocyte nucleus comes into focus. Click Next to move to the next area.
	<ol>
		<li>Classify follicles as a primordial if the oocyte is surrounded by squamous (flattened) granulosa cells, but no cuboidal granulosa cells (Figure 2A). 
		NOTE: Primordial follicles are distinct from intermediate/transitional follicles, which comprise a combination of cuboidal and squamous granulosa cells (Figure 2B), and primary follicles, which are surrounded predominantly by cuboidal granulosa cells (Figure 2C). These follicle classes should be quantified separately.</li>
		<li>Only count follicles in which the oocyte nucleus is visible. The oocyte nucleus must appear within the counting frame or be touching the green inclusion lines of the counting frame (Supplementary Figure 1E,F).</li>
		<li>If the oocyte nucleus falls outside the counting frame (Supplementary Figure 1G) or touches the red exclusion lines of the counting frame, do not count this follicle.</li>
		<li>When assessing primordial follicle depletion in response to an exogenous chemical (e.g., chemotherapy), ensure all follicles counted are healthy and thus have normal morphology (Figure 2). Count any abnormal or atretic follicles separately. Often, follicle death is induced by insults such as chemotherapy, and quantification of the atretic follicles should be obtained separately in order to distinguish between healthy and atretic follicles, as only healthy follicles comprise the ovarian reserve15.</li>
	</ol>
	</li>
	<li>Once counting is complete on that section, do one of the following:
	<ol>
		<li>Click Add New Section, and then return to step 2.3 to set up the next section for counting.</li>
		<li>Click I’ve Finished Counting to end the session. Return the objective to 10x, exit the stereology software and turn off the light source, camera, multi-control unit and computer.</li>
	</ol>
	</li>
	<li>Obtain the sum raw follicle number (Q) from each tissue section sampled from the entire ovary, then using a spreadsheet, use the equation below to obtain the final value from each replicate animal (N)4. 
	<img alt="Optical system magnification formula: N=Q(1/f1)(1/f2)(1/f3), diagram for lens analysis." src="/files/ftp_upload/61782/61782equ01.jpg" data-altupdatedat="1747911167000" data-alt="Equation 1">, where: 
	N = Total estimated number of follicles within the ovary. 
	Q = Raw primordial follicle count. 
	f1 = Sampling interval. Every 3rd section was sampled thus <img alt="Fraction equation showing proportional relationship, mathematical concept, concise formula." src="/files/ftp_upload/61782/61782equ02.jpg" data-altupdatedat="1747911167000" data-alt="Equation 2">. 
	f2 = Relationship between the counting frame (sample area) and stepper, calculated as <img alt="Sample-to-stepper area ratio, fraction formula for semiconductor lithography process analysis." src="/files/ftp_upload/61782/61782equ03.jpg" data-altupdatedat="1747911167000" data-alt="Equation 3">. Since the sample area was 2256 µm2 (47.5 µm x 47.5 µm) and the stepper area was 10000 µm2 (100 µm x 100 µm), <img alt="Equation illustrating frequency calculation, \(f_2=\frac{2256}{10000}\), mathematical formula." src="/files/ftp_upload/61782/61782equ04.jpg" data-altupdatedat="1747911167000" data-alt="Equation 4">. 
	f3 = Fraction of ovarian section sampled. Since 10 µm of the 20 µm section was sampled, <img alt="Equilibrium equation f₃ calculation, algebraic formula for solving fractions, diagram." src="/files/ftp_upload/61782/61782equ05.jpg" data-altupdatedat="1747911167000" data-alt="Equation 5">. 
	Therefore, <img alt="Equation for calculating population growth; involves N=Q(3/1)(10000/2256)(20/10); formula." src="/files/ftp_upload/61782/61782equ06.jpg" data-altupdatedat="1747911167000" data-alt="Equation 6">. 
	NOTE: This protocol describes how to apply these principles of stereological analyses using a widely cited stereology software (Table of Materials); however, other stereological software is available. The principles applied during stereological analyses of ovarian follicles are the same, regardless of the software used to set up the parameters. Stereology is most accurate when 100 or more objects are counted in an adult mouse ovary4, as this gives a coefficient of error for the estimate below 10%16. The sampling parameters outlined here have been optimized to ensure a minimum of approximately 100 objects (i.e., primordial, transitional and primary follicles) can be counted in control adult wild-type C57BL6J ovaries. A pilot study can be conducted including a small sample size to establish the optimal sampling parameters, such as the interval and number of sections to be analyzed and the number of optical dissectors within the sampled sections17.</li>
</ol>
3. Estimation of primordial follicle number by direct ovarian follicle counts
<ol>
	<li>Place the microscope slide securely under a standard light microscope and perform direct counts to obtain raw primordial follicle number.
	<ol>
		<li>Classify follicles as a primordial if the oocyte is clearly visible and is surrounded by squamous (flattened) granulosa cells, but no cuboidal granulosa cells (Figure 2D). 
		NOTE: Primordial follicles are distinct from intermediate/transitional follicles, which comprise a combination of cuboidal and squamous granulosa cells (Figure 2E), and primary follicles, which are surrounded predominantly by cuboidal granulosa cells (Figure 2F). These follicle classes should be quantified separately.</li>
		<li>Ensure all follicles counted are healthy and thus have normal morphology (Figure 2). Count any abnormal or atretic follicles separately, as only healthy follicles comprise the ovarian reserve.</li>
	</ol>
	</li>
	<li>Alternatively, take multiple, or stitched high-power (e.g., 20x) photomicrographs of the entire ovarian tissue section to perform counts by opening the image file(s). This can be done manually, or using an automated slide scanner.</li>
	<li>Obtain the sum raw follicle number (Q) from each tissue section sampled from the entire ovary at the predetermined interval. Multiply this number by the inverse of the sampling fraction to obtain the final value for each replicate animal (N), using the equation below. 
	<img alt="N=Q×(1/f₁) formula, optical system analysis, equation, educational use." src="/files/ftp_upload/61782/61782equ07.jpg" data-altupdatedat="1747911167000" data-alt="Equation 7">, where: 
	N = Total estimated number of follicles within the ovary. 
	Q = Raw follicle count (of each individual type, calculated separately). 
	f1 = Sampling interval. Every 9th section was sampled thus <img alt="Equation showing reciprocals and proportions calculation: f₁ = 1/9, mathematical process." src="/files/ftp_upload/61782/61782equ08.jpg" data-altupdatedat="1747911167000" data-alt="Equation 8">. 
	Therefore, <img alt="N=Q x (9/1) equation for static equilibrium; formula analysis diagram for educational use." src="/files/ftp_upload/61782/61782equ09.jpg" data-altupdatedat="1747911167000" data-alt="Equation 9">.</li>
</ol>

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The authors have nothing to disclose.

This article provides a step-by-step protocol for the gold standard technique for enumerating mouse primordial follicles, stereology, and the more commonly employed method of direct follicle counting. Chemotherapy treatment was used to compare and contrast the results obtained from these two different methods within the left and right ovary from the same animal. Both methods revealed high inter-animal variability in primordial follicle numbers. A significant depletion of the ovarian reserve was recorded using stereology, but direct counting failed to detect a significant reduction in primordial follicle number after chemotherapy administration versus control.
Notably, it is clear that even in an inbred strain of mice, such as C57BL6J, the ovarian reserve in young adult wild type (control) females is widely distributed, as is the case in humans. Factors that influence this and contribute to the establishment of the ovarian reserve remain under investigation18. High variability amongst studies of mouse ovarian function poses numerous challenges for the field to compare, or replicate data and to advance clinical translation of novel therapeutics to protect oocyte number and quality4. This variability is likely due to a number of factors including not only the counting methods employed, but additional factors such as differences between animal strain and age; as well as treatment regimens, such as dose and timing. These factors must all be considered when comparing data from different studies. Regardless, the follicle depletion model employed in this study overall highlights the accurate and sensitive nature of the stereology protocol, whilst also demonstrating that the widely reported direct counts method is unable to detect a known significant primordial follicle depletion.
There are strengths and limitations of each counting method detailed in this article (Table 1). Stereology is regarded as the gold standard method due to its accuracy when used to determine cell number in a variety of different organs5. However, drawbacks of this technique include the time and cost involved, as well as the requirement for specialized equipment and expertise. Together, this has limited the wide-spread use of this procedure for obtaining the most sensitive data.
In contrast, the direct counts method is quick, easy, can be done using archived tissues, and prepared using standard histological techniques. It requires only a light microscope with standard imaging capabilities. However, it does not account for volume changes induced by histological processing, which may disrupt the three-dimensional structure of the ovary. Consequently, follicle morphology is not always adequately preserved, making identification and counting accuracy challenging, especially for inexperienced investigators. While formalin was the fixative used for direct counts in this study, Bouin&#8217;s-fixed tissues can be embedded into paraffin and this may provide better morphology and help researchers to more easily identify primordial follicles. Furthermore, within the literature, sampling fractions for the direct counts method vary widely, ranging from every 3rd to every 10th 5 &#181;m paraffin section19, which may contribute to large discrepancies in follicle counts between studies. Given that paraffin wax sections are so thin, counting every 9th section helps to prevent oversampling and needless counting.
Additional methods not outlined in this guide, but commonly reported in the literature, are counting in only one central section from the entire ovary and considering this to be representative of the entire ovary, or follicle density. This first method is highly problematic, since primordial follicles are not evenly distributed in the ovary and can be found in clusters. This means a single, or even a few sections of the ovary are not representative of the entire organ, making systematic sampling an essential component to any counting method. Follicle density involves counting follicles in an ovarian tissue sample, then expressing the counts per area of tissue. Given the limitations of obtaining primary human tissue, follicle density is often used as a surrogate measure for absolute follicle number in human ovary, though reports in mice are also common. However, this quantification method does not account for the uneven distribution of follicles throughout the ovary, or fluctuations in ovarian volume, which occur routinely throughout the ovarian endocrine (luteal) cycle. This is important because an accurate measure of density amongst samples relies on conserved tissue area. Furthermore, this method often only samples a small biopsy or fraction of the ovary when analyzing human tissues, thus is not representative of the entire ovary. Follicle density lacks the accuracy achievable with stereology. Even using the same whole ovary, comparative measures of follicle quantification following stereological analysis, with follicle density, did not correspond in mouse ovaries20.
Although it is the most commonly used experimental animal, the mouse is only one model species. Obtaining ovaries from larger species, including domestic animals or non-human primates, is possible, thus follicle counts from whole ovarian specimens can be accomplished using a modified stereological protocol21,22. Finally, while the ability to analyze follicle counts in whole human ovaries is indeed very difficult, it nonetheless can be done when specimens are available, using a modified stereological protocol23,24,25.
Future directions in the field may include the expansion and uptake of new techniques. For example, a new methodology of automated detection and counting for primordial follicle oocytes has been described26. This method uses convolutional neural networks driven by labelled datasets and a sliding window algorithm to select test data. However, this algorithm was only tested over two ovaries and widespread uptake remains to be determined. Alternatively, recent advances in optical tissue clearing and light sheet microscopy have permitted comprehensive analysis of intact tissues and some studies have investigated this for follicle enumeration in the mouse ovary27,28.
In conclusion, whilst direct follicle counting is an easy, quick and cost-effective method for enumerating primordial follicles within the ovary, this technique may lack sensitivity, accuracy and be prone to investigator bias. Therefore, despite its drawbacks, stereology remains the best available technique for accurately and reproducibly defining primordial follicle numbers.

The immature, meiotically-arrested oocytes stored within primordial follicles in the ovary are the storage unit for the female germline and comprise an individual&#8217;s lifetime ovarian reserve. Primordial follicle numbers decline naturally with age1, or alternatively, can be prematurely depleted following exposure to exogenous chemicals, including some pharmaceuticals and environmental toxicants in air, food and water2. Given that the primordial follicle number is finite, the quantity and quality of follicles present within the ovary largely determine female fertility and offspring health. Thus, accurate quantification of primordial follicle number in women is essential for evaluating the off-target impacts of exogenous insults on the ovarian reserve.
In women, analysis of the whole ovary is generally not possible, thus non-invasive surrogate measures of the ovarian reserve must be utilized in a clinical setting. Anti-M&#971;llerian hormone (AMH) is the most widely used surrogate biomarker clinically3. Serum AMH levels are often measured in women of advanced maternal age, or before and after cancer treatment, such as chemotherapy. However, AMH is produced by growing follicles and not by primordial follicles, and thus, serum levels do not inform on absolute primordial follicle number.
With the absence of methods to accurately determine primordial follicle number in women in situ, counting ovarian follicles in small animal models, such as rodents, remains an essential research tool to assess the degree by which exogenous insults impact on primordial follicles and thus, fertility. Unfortunately though, reports throughout the literature of primordial follicle numbers in rodent models are highly variable4. A major reason for this is widely reported technical differences in the counting method employed. Predominately, there are two different techniques described in the literature for enumerating primordial follicles in mice. These include stereology, which employs the fractionator optical dissector method, and direct follicle counts.
Stereology is widely regarded the gold standard as it uses systematic uniform random sampling5, making it the most accurate method of quantifying primordial follicle number in whole mouse, or rat ovaries4,6,7. Stereology is unbiased, as it accounts for the three-dimensional structure of the object of interest8. Using an optical dissector/fractionator method, three levels of sampling are applied to quantify primordial follicles using thick tissue sections (e.g., 20 &#181;m) within a known fraction of the total mouse ovary. Firstly, the sampling interval is chosen (e.g., every 3rd section) at a random start (sampling fraction 1, f1)4. Sections are then sampled in a systematic, uniform manner from this point through the whole ovary. Then, an unbiased counting frame is superimposed over the ovarian section and progressively moved along a defined, randomized counting grid (sampling fraction 2, f2)8. Lastly, a known fraction of the section thickness is optically sampled (e.g., 10 &#181;m) and follicles within this area are counted (sampling fraction 3, f3)4. The raw follicle number is multiplied by the inverse of these sampling fractions to obtain the final value. This method requires expert training and equipment, including a microscope with a motorized stage driven by stereological software. Tissues should be preserved in a specialized Bouin&#8217;s fixative, and embedded in glycolmethacrylate resin to allow for thick tissue sections to be cut using a glycolmethacrylate resin microtome with a glass knife. This method is designed to account for tissue shrinkage and deformation, to best preserve the three-dimensional morphological structure of the ovary and follicles9.
Direct follicle counting is the most frequently used method for counting follicles10. More common fixatives (i.e., formalin) can be used, followed by paraffin wax embedding and exhaustive serial sectioning using a standard microtome at a thickness of between 4-6 &#181;m. Follicles are systematically counted in the entire tissue section at a defined interval, and then multiplied by the inverse of the sampling interval to obtain the total follicle estimate. This method is quick, easy, can be performed using archived tissues, and prepared using standard histological techniques. It requires only a light microscope with standard imaging capabilities. However, despite these advantages, direct follicle counting lacks the accuracy and strict counting parameters of stereology, making it more prone to investigator bias. Additionally, tissues may undergo shrinkage and deformation during processing, disrupting the integrity and morphology of the ovary and thus making follicle classification and quantification difficult.
The aim of this article is to describe two commonly-used methods to quantitatively assess primordial follicle number in mouse ovaries: stereology and direct follicle counting. We will provide detailed protocols for these two methods and highlight some of their strengths and weaknesses, in order to enhance reproducibility in our field and allow researchers to make an informed decision of the most appropriate counting method for their studies.

<table><tbody><tr><td>1-Butanol (HPLC)</td><td>Fisher Chemical</td><td>#A383-1</td><td></td></tr><tr><td>Acid alcohol</td><td>Amber Scientific</td><td>#ACDL</td><td></td></tr><tr><td>Bouin&amp;rsquo;s fixative</td><td>Sigma-Aldrich</td><td>#HT10132</td><td>Picric acid 0.9% (w/v), formaldehyde 9% (v/v), acetic acid 5% (w/v)</td></tr><tr><td>Cyclophosphamide</td><td>Sigma-Aldrich</td><td>#C0768-5G</td><td></td></tr><tr><td>Dibutylphthalate Polystyrene Xylene (DPX)</td><td>Sigma-Aldrich</td><td>#06522</td><td></td></tr><tr><td>Ethanol</td><td>Amber Scientific</td><td>#ETH</td><td>Ethanol 100%</td></tr><tr><td>Micro Feather opthalmic scalpel with aluminium handle</td><td>Designs for Vision</td><td>#FEA-745-SR</td><td>Feather blade for dissections (seen in Figure 1)</td></tr><tr><td>Formalin fixative</td><td>Australian Biostain</td><td>#ANBFC</td><td></td></tr><tr><td>Glass coverslip</td><td>Thermo Scientific</td><td>#MENCS22501GP</td><td>22 mm x 50 mm</td></tr><tr><td>Glycomethacrylate resin RM2165 microtome</td><td>Leica Microsystems</td><td>#RM2165</td><td></td></tr><tr><td>Glycolmethacrylate DPX</td><td>*made in house</td><td></td><td>*Mix 1.5 L Xylene; 800 g polystyrene pellets; 100mL Dibutyl phthalate for 3 weeks</td></tr><tr><td>Histolene</td><td>Trajan</td><td>#11031</td><td></td></tr><tr><td>Mayer&amp;rsquo;s haematoxylin</td><td>Amber Scientific</td><td>#MH</td><td></td></tr><tr><td>Olympus BX50 microscope</td><td>Olympus</td><td>#BX50</td><td>Brightfield microscope fitted with 10x dry &amp;amp; 100x oil immersion objective (numerical aperture 1.3)</td></tr><tr><td>Olympus immersion oil type-F</td><td>Olympus</td><td>#IMMOIL-F30CC</td><td></td></tr><tr><td>Olympus TH4-200 light source</td><td>Olympus</td><td>#TH4-200</td><td></td></tr><tr><td>Paraffin wax</td><td>Sigma-Aldrich</td><td>#03987</td><td></td></tr><tr><td>Periodic acid</td><td>Trajan</td><td>#PERI1%</td><td>Periodic acid 1%</td></tr><tr><td>Rotary Microtome CUT 4060</td><td>MicroTec</td><td>#4060R/F</td><td>Used to cut paraffin sections</td></tr><tr><td>Schiff&amp;rsquo;s reagent</td><td>Trajan</td><td>#SCHF</td><td></td></tr><tr><td>Scott&#039;s tap water</td><td>Amber Scientific</td><td>#SCOT</td><td>Potassium carbonate, magnesium sulphate, water</td></tr><tr><td>StereoInvestigator Stereological System</td><td>MBF Bioscience</td><td></td><td>Includes StereoInvestigator software, multi-control unit, automatic stage and joystick</td></tr><tr><td>Superfrost microscope slides</td><td>Thermo Scientific</td><td>#MENSF41296SP</td><td>1 mm, 72 pcs</td></tr><tr><td>Technovit 7100 Plastic embedding system</td><td>Emgrid Australia</td><td>#64709003</td><td>500 mL/5 x 1 g/40 mL</td></tr><tr><td>Technovit 3040 yellow</td><td>Emgrid Australia</td><td>#64708805</td><td>100 g/80 mL</td></tr></tbody></table>

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.

A well-characterized model of follicle depletion was used, whereby young adult female mice were administered a single dose of cyclophosphamide chemotherapy, or saline vehicle control (n=5/group) and both ovaries were harvested from each animal after 48 hours. One ovary per animal was prepared as described in Step 1 for each of the two methods: stereology or direct counts. The left and right ovary from each animal was randomly assigned to each group. These data show that when using stereology, a significant depletion of mouse primordial follicles can be detected following chemotherapy treatment (387 ± 11 follicles), versus control (1043 ± 149; p=0.0024) (Figure 3). In contrast, using the contralateral ovaries from the same animals, direct follicle counts failed to detect a significant reduction of the ovarian reserve after chemotherapy (490 ± 40), when compared to control (752 ± 139; p=0.1063) (Figure 3). Of note, it is clear that primordial follicle number in young adult wild type animals is variable, since the distribution of the saline treated animals is wider, compared to the cyclophosphamide groups, even when counts were performed using stereology (Figure 3).
<img alt="Microtomy process diagram with specimen preparation, cutting equipment, and slide staining setup." class="xfigimg" src="/files/ftp_upload/61782/61782fig01.jpg" data-altupdatedat="1747911167000" data-alt="Figure 1"> 
Figure 1: Histological preparation of Bouin’s-fixed, glycolmethacrylate resin-embedded ovaries for stereological analysis. A) An adult mouse ovary (circle, arrow) was closely trimmed of all fat and the oviduct from the mouse ovary using a Feather blade. B) Contralateral mouse ovaries (circle, arrow) from the same female adult were dissected, trimmed, then either fixed in Bouin’s fixative (left) for stereology, or formalin for direct counts (right). C) A specialized resin methacrylate microtome D) fitted with a glass knife (arrow) was used to exhaustively cut glycolmethacrylate resin blocks into 20 µm sections, collected onto glass microscope slides. E) Periodic acid Schiff-stained ovarian tissue sections on glass microscope slides (arrows) were dipped into fresh histolene (green container) in a fume hood, then a glass coverslip was added on top of drops of GMA DPX. A spatula was used to remove excess DPX and air bubbles. Slides were air dried in the fume hood overnight. <a href="https://www.jove.com/files/ftp_upload/61782/61782fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Cell structure microscopy, six-panel image, highlighting tissue sections and cellular components." class="xfigimg" src="/files/ftp_upload/61782/61782fig02.jpg" data-altupdatedat="1747911167000" data-alt="Figure 2"> 
Figure 2: Primordial follicle classification. Representative images of primordial, transitional and primary follicles in glycolmethacrylate resin-embedded (A-C) and paraffin-embedded (D-F) ovarian sections. A: Primordial follicle surrounded by squamous granulosa cells (arrow). Bar = 10 µm. B: Transitional follicle surrounded by both squamous (arrow) and cuboidal (arrowhead) granulosa cells. Bar = 10 µm. C: Primary follicle surrounded by cuboidal (arrowhead) granulosa cells. Bar = 25 µm. D: Primordial follicle surrounded by squamous granulosa cells (arrow). Bar = 10 µm. E: Transitional follicle surrounded by both squamous (arrow) and cuboidal (arrowhead) granulosa cells. Bar = 10 µm. F: Primary follicle surrounded by cuboidal (arrowhead) granulosa cells. Bar = 25 µm. <a href="https://www.jove.com/files/ftp_upload/61782/61782fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Graph comparing primordial follicle counts using stereology, follicle estimates; saline vs. cyclophosphamide." class="xfigimg" src="/files/ftp_upload/61782/61782fig03.jpg" data-altupdatedat="1747911167000" data-alt="Figure 3"> 
Figure 3: Comparison of the optical fractionator and direct counting methods to evaluate mouse primordial follicles. A well-established model of follicle depletion was used as a model, in which 8-week old female C57BL6J mice were treated intraperitoneally with saline, or a 75 mg/kg/bodyweight dose of the chemotherapeutic, cyclophosphamide (n=6/group). This enabled comparison of the two follicle counting methods to detect changes to the ovarian reserve. In the same cohort of animals, total follicle estimates failed to detect significant follicle depletion, in contrast to stereology which detected a larger and significant depletion of the ovarian reserve. <a href="https://www.jove.com/files/ftp_upload/61782/61782fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td></td>
			<td>STRENGTHS</td>
			<td>WEAKNESSES</td>
		</tr>
		<tr>
			<td rowspan="5">STEREOLOGY</td>
			<td>Most accurate way to estimate follicles</td>
			<td>Time consuming and costly</td>
		</tr>
		<tr>
			<td>Uses several sampling parameters, making it statistically robust</td>
			<td>Requires expert equipment and software</td>
		</tr>
		<tr>
			<td>Highly sensitive, can detect smaller changes in primordial follicle numbers</td>
			<td rowspan="3">Samples must be prepared using specific, specialized histological techniques</td>
		</tr>
		<tr>
			<td>Follicle structure is better preserved during tissue processing</td>
		</tr>
		<tr>
			<td>Uniform rules that can be applied by different investigators, thus reducing bias</td>
		</tr>
		<tr>
			<td rowspan="4">DIRECT COUNTS</td>
			<td>Time and cost effective</td>
			<td>Less accurate and sensitive than stereology</td>
		</tr>
		<tr>
			<td>Requires standard laboratory equipment, e.g. light microscope</td>
			<td>Only one sampling parameter used, making it less effective at detecting small changes in follicle numbers</td>
		</tr>
		<tr>
			<td rowspan="2">Retention of ovarian sections that can be used for immunohistochemical or other analyses</td>
			<td>Tissue is more susceptible to changes in volume and follicle structure during processing</td>
		</tr>
		<tr>
			<td>No uniform set of rules that can be applied, thus more prone to bias from the investigator</td>
		</tr>
	</tbody>
</table>
Table 1: Comparing the strengths and weaknesses of follicle counting methods: stereology vs. direct counts.
Supplementary Figure 1: Screenshots of the stereology software protocol. A) Adjust the exposure by ticking Automatic (red box) under Exposure in the Camera Settings panel (white box). B) Set the white balance by first clicking the More Settings Icon under Other in the Camera Settings panel. Then, select White Balance and click Automatic (red box). C) If an existing sampling configuration has not been set, click No (red box) and enter the serial section information (green box). D) To begin counting, click click Start Counting (white arrow). E) If the nucleus of a primordial follicle is visible within the counting frame, this follicle is counted (white dotted circle). F) If the nucleus of a primordial follicle is touching the green inclusion lines of the counting frame, this follicle is also counted (white dotted circle). G) If the nucleus of a primordial follicle is not visible within the counting frame or is touching the red exclusion lines of the counting frame, this follicle is not counted (white dotted circle). <a href="https://cloudflare.jove.com/files/ftp_upload/61782/61782supfig01.jpg" target="_blank">Please click here to download this figure.</a>
Supplementary Figure 2: Setting up the Sampling Parameters. Follow sequential steps in left-hand panel to define the Probe Configuration. A) Measure mounted thickness. Ensure ‘Refocus to top of section at each grid site’ is unticked (red box). Tick ‘Manually enter the average mounted thickness’ (green box). Enter average mounted thickness as 20.00 µm (blue box). B) Define the counting frame size. Under Counting Frame Display, tick ‘Force the counting frame display to be square’ and ‘Centre on live image’ (red box). Under Counting Frame Size, enter 47.5 µm for X and Y (green box). C) Define SRS grid layout. Manually enter the grid size as 110 for X and Y (red box). D) Define dissector options. For top guard zone height, enter 1.00 µm (red box). For optical dissector height, enter 10 µm (green box). Under Focus Method, select ‘Manual focus’ (blue box). E) Save sampling parameters. To save these settings, enter a Name and Comment then click ‘Save your Current Settings’ (white arrow). F) Under Current Sampling Parameter Settings, ensure your settings match those displayed. <a href="https://cloudflare.jove.com/files/ftp_upload/61782/61782supfig02.jpg" target="_blank">Please click here to download this figure.</a>
Supplementary File 1. <a href="https://cloudflare.jove.com/files/ftp_upload/61782/Supplementary%20Figure%201.ai" target="_blank">Please click here to download this file.</a>
Supplementary File 2. <a href="https://cloudflare.jove.com/files/ftp_upload/61782/Supplementary%20Figure%202.ai" target="_blank">Please click here to download this file.</a>

Watch this Scientific Journal Video about Accurate Follicle Enumeration in Adult Mouse Ovaries at JoVE.com

Accurate Follicle Enumeration in Adult Mouse Ovaries

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

Sexually reproducing female mammals are born with their entire lifetime supply of oocytes. Immature, quiescent oocytes are found within primordial ...

accurate-follicle-enumeration-in-adult-mouse-ovaries

Nanyang Technological University

Research

JoVE Journal

Developmental Biology

8.2K Views.  Monash University. Here, we describe, compare, and contrast two different techniques for accurate follicle counting of fixed mouse ovarian tissues.

Video: Accurate Follicle Enumeration in Adult Mouse Ovaries

Culture and Co-Culture of Mouse Ovaries and Ovarian Follicles

The mammalian ovary is composed of ovarian follicles, each follicle consisting of a single oocyte surrounded by somatic granulosa cells, enclosed together within a basement membrane. A finite pool of follicles is laid down during embryonic development, when oocytes in meiotic arrest form a close association with flattened granulosa cells, forming primordial follicles. By or shortly after birth, mammalian ovaries contain their lifetime&#8217;s supply of primordial follicles, from which point onwards there is a steady release of follicles into the growing follicular pool.
The ovary is particularly amenable to development in vitro, with follicles growing in a highly physiological manner in culture. This work describes the culture of whole neonatal ovaries containing primordial follicles, and the culture of individual ovarian follicles, a method which can support the development of follicles from an immature through to the preovulatory stage, after which their oocytes are able to undergo fertilization in vitro. The work outlined here uses culture systems to determine how the ovary is affected by exposure to external compounds. We also describe a co-culture system, which allows investigation of the interactions that occur between growing follicles and the non-growing pool of primordial follicles.

This protocol describes the primary culture/co-culture of mouse ovarian tissue, using ovaries from neonatal mice and individual ovarian follicles from prepubertal mice. The culture techniques support development in a highly physiological manner, allowing investigation of the effect of extrinsic agents on the ovary, and of interactions between ovarian follicles.

The mammalian ovary is composed of ovarian follicles, each follicle consisting of a single oocyte surrounded by somatic granulosa cells, enclosed together ...

Retrieval of Mouse Oocytes

To date, only a few studies have reported successful manipulations of Peromyscus embryogenesis or reproductive biology.  Together with the Peromyscus Genetic Stock Center (http://stkctr.biol.sc.edu), we are characterizing the salient differences needed to develop this system.  A primary goal has been to optimize oocyte/early embryo retrieval.

This protocol illustrates the technique for extracting oocytes or early-stage fertilized embryos from the oviduct of mice. The ability to identify the infindibulum and insert a blunt end needle into it is essential to correctly performing the procedure.

To date, only a few studies have reported successful manipulations of Peromyscus embryogenesis or reproductive biology.  Together with the Peromyscus ...

Biology

In Vitro Growth of Mouse Preantral Follicles Under Simulated Microgravity

14 day-old mouse ovarian tissue and preantral follicles isolated from same-aged mice were incubated in a simulated microgravity culture system. We quantitatively assessed follicle survival, measured follicle and oocyte diameters, and examined ultrastructure of the oocytes produced from the system. We observed decreased follicle survival, downregulation of expressions of proliferating cell nuclear antigen and growth differentiation factor 9, as indicators for the development of granulosa cells and oocytes, respectively, and oocyte ultrastructural abnormalities under the simulated microgravity condition. The simulated microgravity experimental setup needs to be optimized to provide a model for investigation of the mechanisms involved in the oocyte/follicle in vitro development.

In Vitro Growth of Mouse Preantral Follicles Under Simulated Microgravity

A highly promising technique to generate tissue constructs without using matrix is to culture cells in a simulated microgravity condition. Using a rotary culture system, we examined ovarian follicle growth and oocyte maturation in terms of follicle survival, morphology, growth, and oocyte function under the simulated microgravity condition.

14 day-old mouse ovarian tissue and preantral follicles isolated from same-aged mice were incubated in a simulated microgravity culture system. We ...

A Neural Network-Based Identification of Developmentally Competent or Incompetent Mouse Fully-Grown Oocytes

Infertility clinics would benefit from the ability to select developmentally competent vs. incompetent oocytes using non-invasive procedures, thus improving the overall pregnancy outcome. We recently developed a classification method based on microscopic live observations of mouse oocytes during their in vitro maturation from the germinal vesicle (GV) to the metaphase II stage, followed by the analysis of the cytoplasmic movements occurring during this time-lapse period. Here, we present detailed protocols of this procedure. Oocytes are isolated from fully-grown antral follicles and cultured for 15 h inside a microscope equipped for time-lapse analysis at 37 &#176;C and 5% CO2. Pictures are taken at 8 min intervals. The images are analyzed using the Particle Image Velocimetry (PIV) method that calculates, for each oocyte, the profile of Cytoplasmic Movement Velocities (CMVs) occurring throughout the culture period. Finally, the CMVs of each single oocyte are fed through a mathematical classification tool (Feed-forward Artificial Neural Network, FANN), which predicts the probability of a gamete to be developmentally competent or incompetent with an accuracy of 91.03%. This protocol, set up for the mouse, could now be tested on oocytes of other species, including humans.

Here, we present a protocol for non-invasive assessment of oocyte developmental competence performed during their in vitro maturation from the germinal vesicle to the metaphase II stage. This method combines time-lapse imaging with particle image velocimetry (PIV) and neural network analyses.

Infertility clinics would benefit from the ability to select developmentally competent vs. incompetent oocytes using non-invasive procedures, thus ...

Whole Mount Immunofluorescence and Follicle Quantification of Cultured Mouse Ovaries

Research in the field of mammalian reproductive biology often involves evaluating the overall health of ovaries and testes. Specifically, in females, ovarian fitness is often assessed by visualizing and quantifying follicles and oocytes. Because the ovary is an opaque three-dimensional tissue, traditional approaches require laboriously slicing the tissue into numerous serial sections in order to visualize cells throughout the entire organ. Furthermore, because quantification by this method typically entails scoring only a subset of the sections separated by the approximate diameter of an oocyte, it is prone to inaccuracy. Here, a protocol is described that instead utilizes whole organ tissue clearing and immunofluorescence staining of mouse ovaries to visualize follicles and oocytes. Compared to more traditional approaches, this protocol is advantageous for visualizing cells within the ovary for numerous reasons: 1) the ovary remains intact throughout sample preparation and processing; 2) small ovaries, which are difficult to section, can be examined with ease; 3) cellular quantification is more readily and accurately achieved; and 4) the whole organ imaged.

Here, we present a protocol to quantify follicles in cultured ovaries of young mice without serial sectioning. Using whole organ immunofluorescence and tissue clearing, physical sectioning is replaced with optical sectioning. This method of sample preparation and visualization maintains organ integrity and facilitates automated quantification of specific cells.

Research in the field of mammalian reproductive biology often involves evaluating the overall health of ovaries and testes. Specifically, in females, ...

Ovarian Tissue Culture to Visualize Phenomena in Mouse Ovary

Mammalian females periodically ovulate an almost constant number of oocytes during each estrus cycle. To sustain such regularity and periodicity, regulation occurs at the hypothalamic-pituitary-gonadal axis level and on developing follicles in the ovary. Despite active studies, follicle development mechanisms are not clear because of the several steps involved from the dormant primordial follicle activation to ovulation, and because of the regulation complexity that differs at each follicular stage. To investigate the mechanisms of follicle development, and the dynamics of follicles throughout the estrus cycle, we developed a mouse ovarian tissue culture model that can be used to observe follicle development using a microscope. Systematic follicle development, periodical ovulation, and follicle atresia can all be reproduced in the cultured ovary model, and the culture conditions can be experimentally modulated. Here, we demonstrate the usefulness of this method in the study of the regulatory mechanisms of follicle development and other ovarian phenomena.

Ovarian tissue cultures can be used as models of follicle development, ovulation, and follicle atresia and indicate regulatory mechanisms of dynamic ovarian processes.

Mammalian females periodically ovulate an almost constant number of oocytes during each estrus cycle. To sustain such regularity and periodicity, ...

Whole Ovary Immunofluorescence, Clearing, and Multiphoton Microscopy for Quantitative 3D Analysis of the Developing Ovarian Reserve in Mouse

Female fertility and reproductive lifespan depend on the quality and quantity of the ovarian oocyte reserve. An estimated 80% of female germ cells entering meiotic prophase I are eliminated during Fetal Oocyte Attrition (FOA) and the first week of postnatal life. Three major mechanisms regulate the number of oocytes that survive during development and establish the ovarian reserve in females entering puberty. In the first wave of oocyte loss, 30-50% of the oocytes are eliminated during early FOA, a phenomenon that is attributed to high Long interspersed nuclear element-1 (LINE-1) expression. The second wave of oocyte loss is the elimination of oocytes with meiotic defects by a meiotic quality checkpoint. The third wave of oocyte loss occurs perinatally during primordial follicle formation when some oocytes fail to form follicles. It remains unclear what regulates each of these three waves of oocyte loss and how they shape the ovarian reserve in either mice or humans.
Immunofluorescence and 3D visualization have opened a new avenue to image and analyze oocyte development in the context of the whole ovary rather than in less informative 2D sections. This article provides a comprehensive protocol for whole ovary immunostaining and optical clearing, yielding preparations for imaging using multiphoton microscopy and 3D modeling using commercially available software. It shows how this method can be used to show the dynamics of oocyte attrition during ovarian development in C57BL/6J mice and quantify oocyte loss during the three waves of oocyte elimination. This protocol can be applied to prenatal and early postnatal ovaries for oocyte visualization and quantification, as well as other quantitative approaches. Importantly, the protocol was strategically developed to accommodate high-throughput, reliable, and repeatable processing that can meet the needs in toxicology, clinical diagnostics, and genomic assays of ovarian function.

Here, we present an optimized protocol for imaging entire ovaries for quantitative and qualitative analyses using whole-mount immunostaining, multiphoton microscopy, and 3D visualization and analysis. This protocol accommodates high-throughput, reliable, and repeatable processing that is applicable for toxicology, clinical diagnostics, and genomic assays of ovarian function.

Female fertility and reproductive lifespan depend on the quality and quantity of the ovarian oocyte reserve. An estimated 80% of female germ cells ...

Mouse Oocyte Microinjection, Maturation and Ploidy Assessment

Mistakes in chromosome segregation lead to aneuploid cells. In somatic cells, aneuploidy is associated with cancer but in gametes, aneuploidy leads to infertility, miscarriages or developmental disorders like Down syndrome. Haploid gametes form through species-specific developmental programs that are coupled to meiosis. The first meiotic division (MI) is unique to meiosis because sister chromatids remain attached while homologous chromosomes are segregated. For reasons not fully understood, this reductional division is prone to errors and is more commonly the source of aneuploidy than errors in meiosis II (MII) or than errors in male meiosis 1,2. 
In mammals, oocytes arrest at prophase of MI with a large, intact germinal vesicle (GV; nucleus) and only resume meiosis when they receive ovulatory cues. Once meiosis resumes, oocytes complete MI and undergo an asymmetric cell division, arresting again at metaphase of MII. Eggs will not complete MII until they are fertilized by sperm. Oocytes also can undergo meiotic maturation using established in vitro culture conditions 3. Because generation of transgenic and gene-targeted mouse mutants is costly and can take long periods of time, manipulation of female gametes in vitro is a more economical and time-saving strategy. 
Here, we describe methods to isolate prophase-arrested oocytes from mice and for microinjection. Any material of choice may be introduced into the oocyte, but because meiotically-competent oocytes are transcriptionally silent 4,5 cRNA, and not DNA, must be injected for ectopic expression studies. To assess ploidy, we describe our conditions for in vitro maturation of oocytes to MII eggs. Historically, chromosome-spreading techniques are used for counting chromosome number 6. This method is technically challenging and is limited to only identifying hyperploidies. Here, we describe a method to determine hypo-and hyperploidies using intact eggs 7-8. This method uses monastrol, a kinesin-5 inhibitor, that collapses the bipolar spindle into a monopolar spindle 9 thus separating chromosomes such that individual kinetochores can readily be detected and counted by using an anti-CREST autoimmune serum. Because this method is performed in intact eggs, chromosomes are not lost due to operator error.

Oocytes are prone to aneuploidy due to errors in chromosome segregation during meiotic maturation. Aneuploid eggs can cause infertility, miscarriages or developmental disorders like Down syndrome. Here, we describe methods to introduce materials of choice into oocytes and methods to study meiotic maturation and assess ploidy.

Mistakes in chromosome segregation lead to aneuploid cells.  In somatic cells, aneuploidy is associated with cancer but in gametes, aneuploidy leads to ...

Three-dimensional Reconstruction of the Vascular Architecture of the Passive CLARITY-cleared Mouse Ovary

The ovary is the main organ of the female reproductive system and is essential for the production of female gametes and for controlling the endocrine system, but the complex structural relationships and three-dimensional (3D) vasculature architectures of the ovary are not well described. In order to visualize the 3D connections and architecture of blood vessels in the intact ovary, the first important step is to make the ovary optically clear. In order to avoid tissue shrinkage, we used the hydrogel fixation-based passive CLARITY (Clear Lipid-exchanged Acrylamide-hybridized Rigid Imaging/ Immunostaining/In situ-hybridization-compatible Tissue Hydrogel) protocol method to clear an intact ovary. Immunostaining, advanced multiphoton confocal microscopy, and 3D image-reconstructions were then used for the visualization of ovarian vessels and follicular capillaries. Using this approach, we showed a significant positive correlation (P &#60;0.01) between the length of the follicular capillaries and volume of the follicular wall.

Here we present an adaptation of the passive CLARITY and 3D reconstruction method for visualization of the ovarian vasculature and follicular capillaries in intact mouse ovaries.

The ovary is the main organ of the female reproductive system and is essential for the production of female gametes and for controlling the endocrine ...

Developing an Ovariectomized Mouse Model with Elevated FSH Level

Exploring Independent Effects of Follicle-Stimulating Hormone In Vivo in a Mouse Model

During the transition from a reproductive to a nonreproductive phase (menopause), many women experience significant physiological and pathological changes, including decreased bone mass, increased blood lipids, and increased visceral adiposity. Levels of follicle-stimulating hormone (FSH) rise during the menopausal transition. Many studies have shown that FSH in various extragonadal tissues and organs is associated with the pathogenesis of multiple diseases. Thus, building an animal model that can help study the independent effects of FSH in vivo is particularly important. In this study, C57BL/6 female mice were ovariectomized and supplemented with estradiol valerate (OVX + E2) to eliminate the effect of the hypothalamic-pituitary-gonadal axis. The OVX + E2 mice received solvent (N.S.) or different doses of recombinant FSH via intraperitoneal injection to create a mouse model (OVF) characterized by relatively stable estrogen and rising FSH levels. Thus, we successfully generated an experimental mouse model to mimic the early stage of menopause transition, characterized by elevated serum FSH levels. The OVF model has the advantages of being stable, low cost, and easy to operate, which is suitable for studies to explore the extragonadal actions of FSH. Here, we describe detailed protocols for the mouse OVF model.

Author Spotlight: Investigating the Relationship Between FSH and Pathophysiological Changes in Perimenopausal Women - Insights from a Mouse Model 

Follicle-stimulating hormone (FSH) in various extragonadal tissues and organs is associated with the pathogenesis of multiple diseases. The ovariectomized and FSH-treated mouse model (OVF) can be used to explore the extragonadal actions of FSH.

Accurate Follicle Enumeration in Adult Mouse Ovaries

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Whole Ovary Immunofluorescence, Clearing, and Multiphoton Microscopy for Quantitative 3D Analysis of the Developing Ovarian Reserve in Mouse

Mouse Oocyte Microinjection, Maturation and Ploidy Assessment

Three-dimensional Reconstruction of the Vascular Architecture of the Passive CLARITY-cleared Mouse Ovary

Exploring Independent Effects of Follicle-Stimulating Hormone In Vivo in a Mouse Model