The authors thank Masaki Yoda and Elise Lamar for critical reading of the manuscript, Kazumasa Takenouchi for help with histology, Mari Fujiwara for help with microscopy and Makoto Morikawa for help in photographing human and mouse auditory ossicles.

All animal procedures performed in this study are approved by the Keio University Institutional Animal Care and Use Committee (IACUC - approval number: 09221) and follow the Institutional Guidelines on Animal Experimentation at Keio University for the use of animals in research. Human specimens were isolated from a cadaver donated to the Department of Anatomy, Keio University School of Medicine, and were used in accordance with institutional regulations.
1. Isolation of Auditory Bulla and Capsule
<ol>
	<li>Euthanize mice in a jar containing a platform above paper towels soaked in isoflurane or sevoflurane until respiratory ventilation ceases for more than a min and then perform cervical dislocation. Be careful to avoid direct contact of mice with the soaked paper towels.</li>
	<li>Make a small transverse incision at the dorsal side of the neck and pull skin apart toward the head and tail using both hands to expose underlying neck muscle tissue.</li>
	<li>Decapitate mice at the cervical region using 14&#160;cm sharp surgical scissors.</li>
	<li>Peel skin completely towards the nose. Cut off all skin together with the snout and incisors.</li>
	<li>Insert scissors into the mouth and cut masseter muscles on both sides.</li>
	<li>Open the jaw carefully and remove the tongue and lower jaw together.</li>
	<li>Using sharp scissors, split skull and skull base into two halves along the midsagittal plane (Figure 1A, B).</li>
	<li>Using forceps, remove the cerebral and cerebellar hemispheres and the brainstem. The auditory bulla and capsule are located lateral to the cerebellum and brainstem. Note that the auditory bulla is further lateral to the auditory capsule (Figure 1C, D).</li>
	<li>Dissect out the bulla and capsule with the surrounding skull bone (Figure 1E).</li>
	<li>Transfer the specimen to a dish containing Phosphate-buffered Saline (PBS) pH 7.4 at RT.</li>
	<li>Under a binocular dissecting microscope, use forceps to pull apart the surrounding bones and scissors to cut the loosened boundary around the bulla and capsule (Figure 1F). The surrounding bones removed are the basioccipital (ventral border), exoccipital (ventro-posterior border), supraoccipital (posterior border), interparietal, parietal (dorsal border), squamosal (dorso-anterior border), alisphenoid (anterior border), and basisphenoid (antero-ventral border) bones. Note that the styliform process (Sp), which supports the tympanic opening of the Eustachian tube 41, is distinct from the styloid process of the temporal bone.</li>
</ol>
2. Isolation of Auditory Ossicles: Malleus, Incus and Stapes&#160;
<ol>
	<li>Malleus
	<ol>
		<li>Using both small scissors and forceps, remove the part of the external auditory canal lateral to the sulcus tympanicus so that the tympanic membrane is visible (Figure 2A, B).</li>
		<li>Remove part of the tympanic membrane and tympanic bone near the malleal processus brevis (orbicular apophysis, see Discussion), both at the ventral (dotted) and posterior (#) walls (Figure 2C). The malleus and tensor tympani muscle should now be exposed (Figure 2D, E).</li>
		<li>Lift the malleus (Figure 2F) and cut the tensor tympani muscle with the beveled edge of a 27 G&#160;needle (Figure 2G). Note that the malleal manubrium firmly attaches to the tympanic membrane, as is seen in other mammals.</li>
		<li>Detach the tympanic membrane carefully from the manubrium, which is fragile. Remove the tympanic bone to reveal the three auditory ossicles.</li>
		<li>Dislocate the malleus from the incus at the ossicular joint (Figure 2H).</li>
		<li>Isolate the malleus by fracturing the anterior process at the goniale.</li>
	</ol>
	</li>
	<li>Incus and Stapes
	<ol>
		<li>Isolate the incus by cutting off the posterior ligament of the incus at the short crus (Figure 3A).</li>
		<li>Isolate the stapes by cutting off the stapedial artery near the stapes with the beveled edge of a 27 G&#160;needle (Figure 3B, C). If necessary, cut the tendon of the stapedial muscle at the muscular process of the stapes with the needle.</li>
		<li>Insert a sewing needle (or a marking pin) into the obturator foramen of the stapes and lift up the stapes. After removing the stapes, the oval window opening should be clearly visible (Figure 3D).</li>
	</ol>
	</li>
</ol>
3. Embedding of Auditory Bulla and Capsule
<ol>
	<li>Preparation for embedding in paraffin blocks
	<ol>
		<li>Isolate the bulla and capsule as described in Section 1.</li>
		<li>Cut the anterior end of the bulla (the styliform process) off with scissors, immerse the bulla and capsule in 4% paraformaldehyde (PFA) in PBS at 4 &#176;C, and allow fixative to enter into the bulla. If air becomes trapped in the bulla, remove it with a needle and syringe. Leave the bulla and capsule in the fixative at 4 &#176;C O/N on a tube rotator. 
		Caution: PFA is toxic and should be handled carefully.</li>
		<li>Wash once with PBS.</li>
		<li>Decalcify bulla and capsule for a week at 4 &#176;C in 10% ethylenediaminetetraacetic acid disodium salt dihydrate (EDTA-2Na), 100 mM Tris base, pH 7.0, in a 2 mL tube. Change the buffer every other day.</li>
		<li>Wash once with PBS. Specimens can be stored in 70% ethanol in water at 4 &#176;C. Optionally, transfer to 70% ethanol through a graded alcohol series (30%, 50%, 70% in water).</li>
		<li>On a tissue processor, dehydrate specimens in a graded series of ethanol solutions (70%, 2x 95%, 3x 100%, each 1 h), clear in xylene (4x, each 1 h&#160;at 40 &#176;C), and infiltrate specimens with molten paraffin wax42. Optionally, substitute xylene with commercial tissue clearing solution (e.g., Histo-Clear).</li>
		<li>Unload specimens from the processor, and remove them from their cassettes.</li>
		<li>On a tissue embedding console system, place specimens into molds filled with molten paraffin wax. Proceed to embedding (Section 4).</li>
	</ol>
	</li>
	<li>Preparation for embedding in frozen blocks (Kawamoto&#39;s film method)43
	<ol>
		<li>Isolate the bulla and capsule as described in Section 1.</li>
		<li>Cut the anterior end of the bulla (the styliform process) off with scissors, immerse the bulla and capsule in fixative (2% or 1% PFA rather than 4% in PBS to preserve antigenicity) at 4 &#176;C. If air is trapped in bulla, remove it using a needle and syringe. Leave the bulla and capsule in the fixative at 4 &#176;C O/N on a tube rotator.</li>
		<li>Wash bulla and capsule quickly in PBS and immediately immerse in liquid cryo-embedding compound at 4 &#176;C.</li>
		<li>Important: Remove air bubbles if any in the middle and outer ear through aspiration by a needle, and by adding the embedding compound with forceps. Proceed to embedding (Section 4).</li>
	</ol>
	</li>
</ol>
4. Sample Orientation and Embedding
NOTE: The whole bulla and capsule must be arranged in a particular orientation during embedding to cut desired sections. The procedures outlined below are used to section the malleus in various orientations.
<ol>
	<li>Longitudinal (parasagittal) sectioning of the malleus
	<ol>
		<li>Put the lateral side of the bulla or external auditory meatus down in warm paraffin (or cryo-embedding compound). Adjust the orientation so that the neck and transversal lamina of the malleus are parallel to the horizontal bottom of the embedding dish (Figure 4A - C). Note that the tympanic membrane is inclined at an angle of approximately 30&#176; to the vertical in the mouse head (Figure 4A; Figure 59 in Kampen44).</li>
	</ol>
	</li>
	<li>Horizontal sectioning of the malleus
	<ol>
		<li>Place the dorsal crest horizontally in warm paraffin (or cryo-embedding compound). Adjust the orientation of the bulla and capsule so that the neck and transversal lamina of the malleus are perpendicular to the bottom of the embedding dish (Figure 4D - F).</li>
	</ol>
	</li>
	<li>Frontal sectioning (cross sections) of manubrium and tympanic membrane 5
	<ol>
		<li>Place the malleal manubrium in warm paraffin (or cryo-embedding compound) such that it is perpendicular to the bottom of the embedding dish.</li>
	</ol>
	</li>
	<li>Cool down the block to temperatures appropriate to harden paraffin wax on a tissue embedding console system (alternatively, use cryo-embedding compound in a dry ice/hexane bath).</li>
	<li>Process tissue block and cut sections using routine procedures. For example, stain paraffin sections with hematoxylin and eosin (H&#38;E), safranin O (for cartilage), or for Tartrate-resistant Acid Phosphatase (TRAP) activity (for osteoclasts) 3, or by immunohistochemistry. Undecalcified cryosections are suitable for bone labeling using fluorochromes 14, alizarin red staining for calcium, and immunofluorescence 42.</li>
</ol>

The authors have nothing to disclose.

Here, we present a method useful to isolate the auditory bulla and capsule in postnatal mice. Prior to P12, tissues are fragile and can become damaged during isolation. After P12, the auditory bulla and capsule can be easily isolated from surrounding tissues. Dissecting the bulla from the head before sectioning has several advantages. First, postnatal cavitation and growth of the auditory bulla occur most actively from P6 onwards and are complete by P14 50. The mesenchymal tissue between the tympanic membrane and cochlear wall is replaced by air through the cavitation process. The resultant air in the middle ear cavity can impede contact between tissues and liquids during fixation, decalcification and embedding. It is easier to remove air from the isolated auditory bulla by cutting off the anterior end (styliform process) rather than trying to do so in the unisolated bulla. Second, orientation of the malleus (and the tympanic membrane) is not vertical in the head. It is therefore easier to section the malleus in desired planes by embedding the isolated auditory bulla and capsule in a given orientation.
Once isolated, auditory bulla and capsules are useful for numerous analyses. For example, high resolution X-ray micro-CT can reveal bone microstructure morphology such as osteogenic capillaries in the malleus 14. The stereofluorescence dissecting microscope is a powerful tool to visualize structures in evaluating reporter mice expressing fluorescent proteins in the middle or inner ear 33. In addition, various in vivo or ex vivo fluorescence labeling methods and whole mount immunofluorescence detection could be undertaken. Light sheet fluorescence microscopy is also useful for three-dimensional analysis 51. Although not described here, diverse anatomical structures associated with the auditory bulla and capsule such as peripheral nerves, blood vessels, and the tympanic membrane in the middle ear can also be evaluated using this protocol.
Note that paraffin sectioning requires decalcification of bone tissues before embedding and therefore does not allow analysis of mineralization. By contrast, the Kawamoto film method 43 used to prepare frozen sections can be performed without decalcification and is suitable for mineralization studies using in vivo bone-labeling techniques or special staining such as Alizarin staining. Cryo-sectioning conditions should be optimized according based on mouse age. For example, a less cool temperature inside the cryostat chamber is recommended for older mouse specimens to minimize damage to sections.
In mouse, the correct term for the prominent semi-spherical protrusion of the malleus is &#34;orbicular apophysis&#34;. Nevertheless, the term &#34;processus brevis&#34; has been widely used to indicate the orbicular apophysis for more than two decades, particularly among mouse developmental biologists 16,20,22-25. &#34;Processus brevis&#34; originally referred to the lateral process (processus lateralis), which differs from the orbicular apophysis. In humans, a lateral process resembling a slight conical projection forms the general line of attachment to the tympanic membrane, extending from the manubrium (not seen in Figure&#160;6B, medial view). In mice, the lateral process is also a projection of the manubrium at the opposite end to the umbo 48. The pars flaccida of the tympanic membrane is above the lateral process of the malleus. Orbicular apophysis is not apparent in the human malleus.

The three auditory ossicles of the middle ear, namely the malleus, incus, and stapes, form a mammalian-specific auditory chain that transmits sound from the tympanic membrane to the inner ear, or cochlea 1,2. Hearing function can be evaluated in mice by measuring Auditory Brainstem Response (ABR) thresholds 3-6, and vibration of the malleus behind the tympanic membrane can be monitored using Laser Doppler Vibrometry (LDV) 7. By combining ABR, LDV, and Distortion Product Otoacoustic Emission (DPOAE) measurements, conductive hearing loss can be discriminated from sensorineural impairment 8.
Animal models of ear conditions are needed, given the importance of hearing and ear health to the well-being of patients of all ages. For example, otitis media is an extremely common ear infection seen in human infants and children, and severe, acute otitis media and its complications can occur if the condition is not treated with appropriate antimicrobials 9. Mouse models of otitis media could prove useful in understanding the pathogenesis and in developing treatments 10,11.
Murine ossicles, which (except for the goniale part of the malleus) are formed by endochondral ossification 12,13, are highly relevant to the study of bone metabolism and morphogenesis. First, their small size allows high-resolution analysis of bones with an intact periosteum using X-ray or fluorescence microscopy 14. Second, aberrant bone metabolism, such as excessive or deficient bone resorption, or impaired interactions among bone cells 15, can be analyzed as a potential contributor to hearing loss 3,4,7. Third, abnormal ossicle morphogenesis is reported in several gene-deficient mice, such as animals lacking Hoxa2 16-19, Msx1 20-22, Prrx1 23, Goosecoid (Gsc) 24,25, Bapx1 13, Tshz1 26, Dusp6 (Mkp3) 27, Noggin (Nog) 28, Fgfr1 29, thyroid hormone receptors (Thra, Thrb) 5, Bcl2 30 and others 1,31, or in mice overexpressing Hoxa2 32. Finally, despite their small size, structures associated with ossicles such as muscles 33 and joints 34,35 are accessible.
Mouse ossicles are smaller than human ossicles, but it is noteworthy that the mouse middle ear is not a miniature version of its human counterpart. For example, in mice, the stapedial artery, which passes through the ring of the stapes, persists throughout life 36, whereas in humans, the embryonic stapedial artery disappears during gestation. In addition, the morphology of the mouse malleus differs from that of the human bone (see Figure 6). In mice, the auditory (tympanic) bulla encloses the air-filled middle ear cavity, whereas in humans, mastoid air cells composed of trabecular bone in the temporal bone houses the ossicles rather than a bulla 37. In both species, the auditory capsule (otic capsule, bony labyrinth) encloses the cochlea and semicircular canals of the inner ear. Comparative and evolutionary biology of the middle ear has been extensively reviewed 38-40.
The protocol provided below first describes how to dissect out the auditory bulla and capsule, which consist primarily of the middle ear and inner ear, respectively. This protocol also demonstrates how to isolate the malleus, incus and stapes from the auditory bulla. Finally, it shows how to orient the auditory bulla and capsule for embedding in preparation for tissue sectioning of auditory ossicles.

<table><tbody><tr><td>&lt;strong&gt;Tools/Equipment&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Paper towel</td><td>Daio Paper Corporation</td><td>703347</td><td>can be purchased from other vendors</td></tr><tr><td>Glass Jar</td><td>Various</td><td></td><td>can be purchased from other vendors</td></tr><tr><td>14 cm surgical scissors</td><td>Fine Science Tools (F.S.T.)</td><td>91400-14</td><td>can be purchased from other vendors</td></tr><tr><td>Extra fine scissors-straight</td><td>Fine Science Tools (F.S.T.)</td><td>14084-08</td><td>can be purchased from other vendors</td></tr><tr><td>Fine Forceps Angled 45&lt;b&gt;&amp;deg;&lt;/b&gt;</td><td>Fine Science Tools (F.S.T.)</td><td>11063-07</td><td>can be purchased from other vendors</td></tr><tr><td>Dissecting microscope</td><td>Nikon</td><td>SMZ800N</td><td>for routine dissection</td></tr><tr><td>Dissecting microscope</td><td>Nikon</td><td>SMZ18</td><td>for movies&amp;nbsp;</td></tr><tr><td>Injection needle 27 G</td><td>TERUMO</td><td>NN-2719S</td><td></td></tr><tr><td>Syringe (1 mL)</td><td>TERUMO</td><td>SS-01T</td><td></td></tr><tr><td>Marking Pin</td><td>Various</td><td></td><td></td></tr><tr><td>Tube rotator RT-50</td><td>TAITEC</td><td>0000165-000</td><td>can be purchased from other vendors</td></tr><tr><td>Cryostat</td><td>Leica</td><td>CM3050S</td><td>http://www.leicabiosystems.com/histology-equipment/cryostats/details/product/leica-cm3050-s/</td></tr><tr><td>TC-65 Tungsten blade</td><td>Leica</td><td>14021626379</td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Stainless containers</td><td>Leica</td><td></td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Cryofilm type IIC</td><td>Leica</td><td></td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Silane coated slide (New Silane II)</td><td>Muto Pure Chemicals</td><td>511617</td><td>can be purchased from other vendors</td></tr><tr><td>Cover glass</td><td>Matsunami</td><td></td><td>can be purchased from other vendors</td></tr><tr><td>Tissue processor</td><td>Sakura Finetek</td><td>VIP-5</td><td>can be purchased from other vendors</td></tr><tr><td>Tissue Embedding Console System</td><td>Sakura Finetek</td><td>Tissue-Tek TEC 5&amp;nbsp;</td><td>can be purchased from other vendors</td></tr><tr><td>Sliding microtome for paraffin</td><td>Yamato Kohki Industrial</td><td>REM-710</td><td>can be purchased from other vendors</td></tr><tr><td>Path Blade+pro for hard tissue</td><td>Matsunami</td><td>PB3503C</td><td>for paraffin section</td></tr><tr><td>Micro-CT</td><td>RIGAKU</td><td>R_mCT2</td><td>http://www.rigaku.com/en</td></tr><tr><td>Fluorescence microscope</td><td>KEYENCE</td><td>BZ-9000</td><td></td></tr><tr><td>&lt;strong&gt;Name&lt;/strong&gt;</td><td>&lt;strong&gt;Company&lt;/strong&gt;</td><td>&lt;strong&gt;Catalog Number&lt;/strong&gt;</td><td>&lt;strong&gt;Comments&lt;/strong&gt;</td></tr><tr><td>&lt;strong&gt;Reagents&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Isoflurane</td><td>Maruishi pharmaceutical Co. Ltd</td><td></td><td></td></tr><tr><td>NaCl</td><td>wako</td><td>191-01665</td><td>for PBS</td></tr><tr><td>KCl</td><td>wako</td><td>285-14</td><td>for PBS</td></tr><tr><td>Na&lt;sub&gt;2&lt;/sub&gt;HPO&lt;sub&gt;4&lt;/sub&gt; 12H&lt;sub&gt;2&lt;/sub&gt;O</td><td>wako</td><td>196-02835</td><td>for PBS</td></tr><tr><td>KH&lt;sub&gt;2&lt;/sub&gt;PO&lt;sub&gt;4&lt;/sub&gt;</td><td>wako</td><td>287-21</td><td>for PBS</td></tr><tr><td>Paraformaldehyde (PFA, EM Grade)</td><td>TAAB</td><td>P001</td><td></td></tr><tr><td>EDTA-2Na</td><td>wako</td><td>15111-45</td><td></td></tr><tr><td>Trizma base</td><td>Sigma</td><td>T1503-1KG</td><td></td></tr><tr><td>Super Cryoembedding Medium</td><td>Leica</td><td></td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Dry Ice</td><td>Various</td><td></td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Hexane</td><td>wako</td><td>080-03423</td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Super Cryomouting Medium type R2</td><td>Leica</td><td></td><td>for Kawamoto&#039;s firm method</td></tr><tr><td>Paraffin</td><td>Sakura Finetek</td><td>781001A0107</td><td></td></tr><tr><td>Histo-Clear</td><td>NDS</td><td>HS-200</td><td></td></tr><tr><td>Calcein</td><td>DOJINDO</td><td>340-00433</td><td></td></tr><tr><td>Hematoxylin&amp;nbsp;</td><td>wako</td><td>131-09665</td><td></td></tr><tr><td>Eosin</td><td>wako</td><td>051-06515</td><td></td></tr></tbody></table>

dissection of the auditory bulla in postnatal mice: isolation of the middle ear bones and histological analysis

In most mammals, auditory ossicles in the middle ear, including the malleus, incus and stapes, are the smallest bones. In mice, a bony structure called the auditory bulla houses the ossicles, whereas the auditory capsule encloses the inner ear, namely the cochlea and semicircular canals. Murine ossicles are essential for hearing and thus of great interest to researchers in the field of otolaryngology, but their metabolism, development, and evolution are highly relevant to other fields. Altered bone metabolism can affect hearing function in adult mice, and various gene-deficient mice show changes in morphogenesis of auditory ossicles in utero. Although murine auditory ossicles are tiny, their manipulation is feasible if one understands their anatomical orientation and 3D structure. Here, we describe how to dissect the auditory bulla and capsule of postnatal mice and then isolate individual ossicles by removing part of the bulla. We also discuss how to embed the bulla and capsule in different orientations to generate paraffin or frozen sections suitable for preparation of longitudinal, horizontal, or frontal sections of the malleus. Finally, we enumerate anatomical differences between mouse and human auditory ossicles. These methods would be useful in analyzing pathological, developmental and evolutionary aspects of auditory ossicles and the middle ear in mice.

This protocol presents a method to isolate ossicles from the mouse auditory bulla. First, the bulla and capsule are dissected out as a single piece from the skull (Figure 1). The dissected bulla is then used to prepare the malleus (Figure 2) and the incus and stapes (Figure 3). Landmarks of the auditory bulla and capsule are the styliform process at the anterior end of the bulla, the dorsal crest, anterior semicircular canal, and the subarcuate fossa (Figure 1F). Microcomputed tomography (CT) imaging reveals ossicles in the auditory bulla as well as the optimal orientations for longitudinal and horizontal sectioning of those ossicles (Figure 4).
For longitudinal paraffin sectioning of the malleus, the bulla and capsule were decalcified in EDTA at 4 °C for one week, embedded in a paraffin block at the orientation shown in Figure 4 A - C, sectioned at 4 µm, and then stained using H&amp;E. The malleus attached to the tympanic membrane in the auditory bulla revealed ongoing endochondral ossification at P14 (Figure 5A). To visualize new bone formation, calcein (30 µg/g bodyweight) was peritoneally injected into a P20 mouse, and bulla and capsule were isolated 24 h later at P21. The sample without decalcification was embedded frozen and then cryosectioned at 6 µm using an adhesive film based on the method of Kawamoto 43. After nuclear staining with DAPI (4',6-diamidino-2-phenylindole), the section was observed under a fluorescence microscope. Calcein signals (green) revealed new bone formation in the malleus (m), bulla and capsule (Figure 5B). For horizontal sectioning of the malleus, the auditory bulla isolated from a 5-week-old mouse was embedded frozen without decalcification (for the orientation see Figure 4D - F), cryosectioned at 6 µm using the Kawamoto method, and stained using H&amp;E. Horizontal sectioning of the malleal processus brevis (mPB) also shows the cochlea (Figure 5C).
A medial view of the right auditory ossicles isolated from a P31 mouse shows typical features of the mouse malleus, namely, the "gliding-seagull-wing-like" (or Persian sword-like 45) manubrium, a prominent processus brevis (orbicular apophysis, see Discussion), and the transversal lamina (Figure 6). Note that the anterior process (processus anterior) was fractured in the dissection procedure around the goniale and was separated from the tympanic ring (ectotympanic). This representative sample exhibits an intact incudomalleolar joint between the malleus and incus, whereas the incudostapedial joint is dislocated. Tendinous insertions into the malleal and stapedial muscular processes are detectable (Figure 6A, asterisks).
Figure 6B compares mouse and human auditory ossicles at the same magnification. Species differences, other than size, include the following. The malleal manubrium is wing-like in mice but club-like in humans. The angle between the anatomical axis (or the axis of rotation, the line through the anterior process of the malleus and the short process of the incus) and the manubrium is much smaller in mice and the two are almost parallel, as opposed to nearly perpendicular in humans 6,46-48. In human ossicles, vibrometric studies reveal that the incudo-malleolar joint is mobile rather than functionally fixed 49. The mouse malleus exhibits a wide, thin, and flat transversal lamina not apparent in humans 47. In mice, the processus anterior fuses to membranous bones, namely the goniale and the tympanic ring, while in humans the processus anterior is reduced to a small spicule of bone 41. The stapes of mice and humans also differs: in mice, the anterior crus is curved and the posterior crus is more straight whereas in humans, the anterior crus is more straight than the posterior crus. It is worth noting that the malleus head relative to body size is massively enlarged in species such as the golden mole, demonstrating significant variability in allometric relationships of "the smallest" bones 48.
<img alt="Neuroanatomy dissection process; annotated tissue samples, directional markers; educational analysis." src="/files/ftp_upload/55054/55054fig1.jpg" data-altupdatedat="1747911167000" data-alt="Figure 1"> 
Figure 1. Dissection of the Auditory Bulla and Capsule. (A) The skull of a P31 mouse is split into right and left halves. A, anterior; P, posterior; L, left; R, right. (B) Medial surface of the right half of the bisected, skinned head. Cx, cerebral cortex; Cb, cerebellum; Bs, brainstem. D, dorsal; V, ventral. (C) Removal of brain with forceps. (D) Medial view of the auditory capsule in the right skull. The dorsal crest (arrowheads) lies between the middle cranial fossa (mcf) and posterior cranial fossa (pcf) and separates dorso-anterior and ventro-posterior surfaces of the auditory capsule. Scale bar, 2 mm. (E) Higher magnification of auditory bulla and capsule (medial view). Co, cochlea; VII, facial nerve; VIII, vestibulocochlear nerve; AC, anterior (superior) semicircular canal; Sf, subarcuate fossa, which houses the cerebellar paraflocculus. Scale bar, 1 mm. (F) Micrograph of isolated auditory bulla and capsule (medial view). Sp, styliform process. Scale bar, 1 mm. (A - E), P31 mouse. (F), P33 mouse. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Mollusk anatomy diagrams with labeled structures for educational research on shell development." src="/files/ftp_upload/55054/55054fig2.jpg" data-altupdatedat="1747911167000" data-alt="Figure 2"> 
Figure 2. Dissection of the Malleus. (A) Ventrolateral view of a right auditory bulla and capsule. The sulcus tympanicus (ST, dashed arrow) is the attachment site of the tympanic membrane. The bone lateral to the ST is part of the external ear, and the bone medial to the ST forms the floor of the middle ear cavity. A, anterior; P, posterior; D, dorsal; V, ventral. (B) View after removal of the external auditory canal to reveal the tympanic membrane (TM) including the pars flaccida (Pf) and pars tensa (Pt). (C) Removal of parts of the tympanic bone (dotted lines and #) near the malleal processus brevis (mPB). m, malleus; mM, malleal manubrium. Arrow, air bubble in the middle ear cavity seen through the tympanic membrane. (D) Exposed malleus. Malleus head is indicated. Dotted line indicates the articular surface of the incus. (E) Tendon of the tensor tympani muscle (TT) attached to the malleus. (F) The tensor tympani is pulled when the malleus is lifted. *, muscular process. (G) Tensor tympani is cut using a needle. (H) Three auditory ossicles after removal of the tympanic membrane. The incudo-malleolar joint is dislocated. m, malleus; i, incus; s, stapes; Go, goniale (fused to the malleus and tympanic ring, TR). All scale bars, 0.5 mm. (A, H), P33 mouse. (B - G), P31 mouse. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Microscopic anatomy diagram, auditory system structures labeled: IC, OW, RW; study of sound pathways." src="/files/ftp_upload/55054/55054fig3.jpg" data-altupdatedat="1747911167000" data-alt="Figure 3"> 
Figure 3. Dissection of the Incus and Stapes. (A) Incus and stapes after removal of the malleus. The stapedial artery (SA) passes through the stapes (s). Dotted line indicates the articular surface of the incus. Note that the short crus (iCB, crus breve) of the incus (i) is fixed by the posterior ligament (not shown). Asterisk, muscular process of the stapes. (B) Stapes after removal of the incus. Needle tip is used to cut the stapedial artery (SA). Arrow, direction of blood flow. Dotted line indicates articular surface of the stapes. (C) The stapedial artery is removed from the stapes. X indicates the cut end of the stapedial artery (SA). (D) The oval window (Ow, fenestra ovalis or fenestra vestibuli) is visible after removal of the stapes. Rw, round window (fenestra rotunda or fenestra cochleae). Scale bars, 0.5 mm. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Fluorescence microscopy images highlighting anatomical features in longitudinal and horizontal sections." src="/files/ftp_upload/55054/55054fig4.jpg" data-altupdatedat="1747911167000" data-alt="Figure 4"> 
Figure 4. Orienting the Auditory Bulla and Capsule during Embedding for Longitudinal (parasagittal, A - C) and Horizontal (D - E) Sectioning of the Malleus. (A - C) The neck and transversal lamina of the malleus are placed parallel to the bottom of embedding dish. (A) Side view: micro-CT image to show embedding of the right malleus in the bulla (pseudocolored blue). The malleus and incus are pseudocolored green. Dashed line, the desired cutting plane. Solid line, bottom of embedding dish. m, malleus; arrowheads, dorsal crest. M, medial; L, lateral; D, dorsal; V, ventral. (B) Top view: Micro-CT image. Note that the anterior end of the bulla (styliform process) was removed. i, incus. (C) Top view: micrograph (taken with a color filter). AC, anterior (superior) semicircular canal; Sf, subarcuate fossa; Sp, styliform process. A, anterior; P, posterior; D, dorsal; V, ventral. (D - F) The processus brevis of the malleus is placed perpendicular to the bottom of embedding dish. (D) Side view: Micro-CT image to show embedding of the right malleus. Dashed line, the desired cutting plane. Solid line, bottom of embedding dish. (E) Top view: Micro-CT image. mM, malleal manubrium. (F) Top view: micrograph (taken with a color filter). Scale bars, 1 mm. Micro-CT images were obtained at a voxel resolution of 5 μm, as previously described 7. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Histological sections of bone development: paraffin H&amp;E, cryo calcein staining, longitudinal sections." src="/files/ftp_upload/55054/55054fig5.jpg" data-altupdatedat="1747911167000" data-alt="Figure 5"> 
Figure 5. Histology. (A) H&amp;E staining. Longitudinal (parasagittal) section of the paraffin-embedded right malleus (m) in the auditory bulla (dotted line) at P14. TM, tympanic membrane. (B) Calcein bone labeling. Longitudinal section of the frozen, undecalcified left malleus (m) in the auditory bulla at P21. Counterstain, DAPI. (C) H&amp;E staining. Horizontal section of the frozen, undecalcified left malleal processus brevis (mPB) in the auditory bulla and capsule (5-week-old mouse). Co, cochlea. Scale bars, 1 mm. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Anatomical structure diagram with labeled components; vertebrate study setup." src="/files/ftp_upload/55054/55054fig6.jpg" data-altupdatedat="1747911167000" data-alt="Figure 6"> 
Figure 6. Medial View of Auditory Ossicles. (A) Right auditory ossicles of P31 mouse. A, anterior; P, posterior; D, dorsal; V, ventral. Scale bar, 1 mm. malleus head (Caput mallei, Capitulum mallei); neck (Collum mallei); lamina (transversal lamina); mM (Manubrium mallei); black asterisk (muscular process of the malleus); mPA (Processus anterior, Processus gracilis); mPB (processus brevis); incus body (Corpus incudis); iCB (Crus breve, short crus, short process); iCL (Crus longum, long crus, long process); iPL (Processus lenticularis, lenticular process, Sylvian apophysis); stapes head (Caput stapedis); white asterisk (muscular process of the stapes); sCA (Crus anterius, anterior crus); sCP (Crus posterius, posterior crus); base (Basis stapedis, footplate); sOF (obturator foramen, intercrural foramen). (B) Right auditory ossicles of a 76-year-old human female (Courtesy of Department of Anatomy, Keio University School of Medicine). The ossicles of P31 mouse (lower right) are imaged at the same magnification as that used for human ossicles. Curved arrows indicate the angle between the anatomical axis and the manubrium (dotted lines). Scale bar, 2 mm. <a href="http://cloudflare.jove.com/files/ftp_upload/55054/55054fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Dissection of the Auditory Bulla in Postnatal Mice: Isolation of the Middle Ear Bones and Histological Analysis at JoVE.com

Dissection of the Auditory Bulla in Postnatal Mice: Isolation of the Middle Ear Bones and Histological Analysis

We present a protocol to isolate the auditory bulla, capsule, and ossicles from postnatal mice for whole mount and histological analysis.

In most mammals, auditory ossicles in the middle ear, including the malleus, incus and stapes, are the smallest bones. In mice, a bony structure called ...

dissection-auditory-bulla-postnatal-mice-isolation-middle-ear-bones

Research

JoVE Journal

Biology

30.0K Views.  Keio University School of Medicine. We present a protocol to isolate the auditory bulla, capsule, and ossicles from postnatal mice for whole mount and histological analysis. 

Video: Dissection of the Auditory Bulla in Postnatal Mice: Isolation of the Middle Ear Bones and Histological Analysis

A Protocol for Decellularizing Mouse Cochleae for Inner Ear Tissue Engineering

In mammals, mechanosensory hair cells that facilitate hearing lack the ability to regenerate, which has limited treatments for hearing loss. Current regenerative medicine strategies have focused on transplanting stem cells or genetic manipulation of surrounding support cells in the inner ear to encourage replacement of damaged stem cells to correct hearing loss. Yet, the extracellular matrix (ECM) may play a vital role in inducing and maintaining function of hair cells, and has not been well investigated. Using the cochlear ECM as a scaffold to grow adult stem cells may provide unique insights into how the composition and architecture of the extracellular environment aids cells in sustaining hearing function. Here we present a method for isolating and decellularizing cochleae from mice to use as scaffolds accepting perfused adult stem cells. In the current protocol, cochleae are isolated from euthanized mice, decellularized, and decalcified. Afterward, human Wharton&#39;s jelly cells (hWJCs) that were isolated from the umbilical cord were carefully perfused into each cochlea. The cochleae were used as bioreactors, and cells were cultured for 30 days before undergoing processing for analysis. Decellularized cochleae retained identifiable extracellular structures, but did not reveal the presence of cells or noticeable fragments of DNA. Cells perfused into the cochlea invaded most of the interior and exterior of the cochlea and grew without incident over a duration of 30 days. Thus, the current method can be used to study how cochlear ECM affects cell development and behavior.

The goal of this protocol is to demonstrate an effective method to decellularize and decalcify mouse cochleae for utilization as scaffolds for tissue engineering applications.

In mammals, mechanosensory hair cells that facilitate hearing lack the ability to regenerate, which has limited treatments for hearing loss. Current ...

Bioengineering

Whole Mount Dissection and Immunofluorescence of the Adult Mouse Cochlea

The organ of Corti, housed in the cochlea of the inner ear, contains mechanosensory hair cells and surrounding supporting cells which are organized in a spiral shape and have a tonotopic gradient for sound detection. The mouse cochlea is approximately 6 mm long and often divided into three turns (apex, middle, and base) for analysis. To investigate cell loss, cell division, or mosaic gene expression, the whole mount or surface preparation of the cochlea is useful. This dissection method allows visualization of all cells within the organ of Corti when combined with immunostaining and confocal microscopy to image cells at different planes in the z-axis. Multiple optical cross-sections can also be obtained from these z-stack images. In addition, the whole mount dissection method can be used for scanning electron microscopy, although a different fixation method is needed. Here, we present a method to isolate the organ of Corti as three intact cochlear turns (apex, middle, and base). This method can be used for mice ranging from one week of age through adulthood and differs from the technique used for neonatal samples where calcification of the cochlea is incomplete. A slightly modified version can be used for dissection of the rat cochlea. We also demonstrate a procedure for immunostaining with fluorescently tagged antibodies.

We present a method to isolate the adult organ of Corti as three intact cochlear turns (apex, middle, and base). We also demonstrate a procedure for immunostaining with fluorescently tagged antibodies. Together these techniques allow the study of hair cells, supporting cells, and other cell types found in the cochlea.

The organ of Corti, housed in the cochlea of the inner ear, contains mechanosensory hair cells and surrounding supporting cells which are organized in a ...

Neuroscience

The Mouse Round-window Approach for Ototoxic Agent Delivery: A Rapid and Reliable Technique for Inducing Cochlear Cell Degeneration

Investigators have utilized a wide array of animal models and investigative techniques to study the mammalian auditory system. Much of the basic research involving the cochlea and its associated neural pathways entails exposure of model cochleae to a variety of ototoxic agents. This allows investigators to study the effects of targeted damage to cochlear structures, and in some cases, the self-repair or regeneration of those structures. Various techniques exist for delivery of ototoxic agents to the cochlea. When selecting a particular technique, investigators must consider a number of factors, including the induction of inadvertent systemic toxicity, the amount of cochlear damage produced by the surgical procedure itself, the type of lesion desired, animal survivability, and reproducibility/reliability of results. Currently established techniques include parenteral injection, intra-peritoneal injection, trans-tympanic injection, endolymphatic sac injection, and cochleostomy with perilymphatic perfusion. Each of these methods has been successfully utilized and is well described in the literature; yet, each has various shortcomings. Here, we present a technique for topical application of ototoxic agents directly to the round window niche. This technique is non-invasive to inner ear structures, produces rapid onset of reliably targeted lesions, avoids systemic toxicity, and allows for an intra-animal control (the contra-lateral ear). Results stemming from this approach have helped deeper understanding of auditory pathophysiology, cochlear cell degeneration, and regenerative capacity in response to an acute injury. Future investigations may use this method to conduct interventional studies involving gene therapy and stem cell transplantation to combat hearing loss.

Various methods exist for introducing ototoxic agents to the cochleae of animal models. Presented is a surgical protocol for delivery of ototoxic agents to the round window niche. The procedure is reliable, creates targeted intra-cochlear lesions, and avoids mechanical damage to the microarchitecture. Examination of cochlear self-repair/regeneration is possible.

Investigators have utilized a wide array of animal models and investigative techniques to study the mammalian auditory system. Much of the basic research ...

Medicine

Evaluation of Planar-Cell-Polarity Phenotypes in Ciliopathy Mouse Mutant Cochlea

In recent years, primary cilia have emerged as key regulators in development and disease by influencing numerous signaling pathways. One of the earliest signaling pathways shown to be associated with ciliary function was the non-canonical Wnt signaling pathway, also referred to as planar cell polarity (PCP) signaling. One of the best places in which to study the effects of planar cell polarity (PCP) signaling during vertebrate development is the mammalian cochlea. PCP signaling disruption in the mouse cochlea disrupts cochlear outgrowth, cellular patterning and hair cell orientation, all of which are affected by cilia dysfunction. The goal of this protocol is to describe the analysis of PCP signaling in the developing mammalian cochlea via phenotypic analysis, immunohistochemistry and scanning electron microscopy. Defects in convergence and extension are manifested as a shortening of the cochlear duct and/or changes in cellular patterning, which can be quantified following dissection from developing mouse mutants. Changes in stereociliary bundle orientation and kinocilia length or positioning can be observed and quantitated using either immunofluorescence or scanning electron microscopy (SEM). A deeper insight into the role of ciliary proteins in cellular signaling pathways and other biological phenomena is crucial for our understanding of cellular and developmental biology, as well as for the development of targeted treatment strategies.

Primary cilia influence various signaling pathways. The mammalian cochlea is ideal for examining planar cell polarity (PCP) signaling. Cilia dysfunction affects cochlear outgrowth, cellular patterning and hair cell orientation, readouts of PCP. Our goal is to analyze PCP signaling in mouse cochlea via phenotypic analysis, immunohistochemistry and scanning electron microscopy.

In recent years, primary cilia have emerged as key regulators in development and disease by influencing numerous signaling pathways. One of the earliest ...

Cryosectioning and Immunostaining Mouse Inner Ear Tissue: From Embryonic to Adult Stages

This protocol details general histology methods for preparing inner ear samples from embryonic, neonatal, and adult mice. The purpose of this protocol is to provide a straightforward and standardized method for inner ear tissue processing for researchers, possibly new to the field, interested in working with the mouse cochlea. Included here are protocols for dissection, fixation, embedding, cryosectioning, and immunostaining. Section immunostaining is one of the best methods for examining individual cells within the context of the entire cochlea.
Key steps include dissecting the inner ear away from the skull, fixing the tissue using 4% paraformaldehyde, embedding with Optimal Cutting Temperature compound, cryosectioning, and immunostaining with antibodies targeting specific proteins expressed by the cochlea.
Included in our methods are special considerations made for the cochlea given its 
shape and structure.&#160;Reasonably good focus and dissection skills are needed, as tissue damage can affect the quality of immunostaining and consistency among samples. However, with the procedures we outline, most users can be trained in a few weeks to make beautiful preparations. Overall, this protocol offers a valuable way to promote research to understand auditory development, function, and disease in mouse models.

This protocol, intended for novice users of mouse inner ear tissue, comprehensively details steps for processing mouse inner ears at different developmental stages for section immunostaining.

This protocol details general histology methods for preparing inner ear samples from embryonic, neonatal, and adult mice. The purpose of this protocol is ...

Developmental Biology

Cochlear Implant Surgery and Electrically-evoked Auditory Brainstem Response Recordings in C57BL/6 Mice

Cochlear implants (CIs) are neuroprosthetic devices that can provide a sense of hearing to deaf people. However, a CI cannot restore all aspects of hearing. Improvement of the implant technology is needed if CI users are to perceive music and perform in more natural environments, such as hearing out a voice with competing talkers, reflections, and other sounds. Such improvement requires experimental animals to better understand the mechanisms of electric stimulation in the cochlea and its responses in the whole auditory system. The mouse is an increasingly attractive model due to the many genetic models available. However, the limited use of this species as a CI model is mainly due to the difficulty of implanting small electrode arrays. More details about the surgical procedure are therefore of great interest to expand the use of mice in CI research.
In this report, we describe in detail the protocol for acute deafening and cochlear implantation of an electrode array in the C57BL/6 mouse strain. We demonstrate the functional efficacy of this procedure with electrically-evoked auditory brainstem response (eABR) and show examples of facial nerve stimulation. Finally, we also discuss the importance of including a deafening procedure when using a normally hearing animal. This mouse model provides a powerful opportunity to study genetic and neurobiological mechanisms that would be of relevance for CI users.

Animal models of cochlear implants can advance knowledge of the technological bases of treating permanent sensorineural hearing loss with electrical stimulation. This study presents a surgical protocol for acute deafening and cochlear implantation of an electrode array in mice as well as the functional assessment with auditory brainstem response.

Cochlear implants (CIs) are neuroprosthetic devices that can provide a sense of hearing to deaf people. However, a CI cannot restore all aspects of ...

Morphological and Functional Evaluation of Ribbon Synapses at Specific Frequency Regions of the Mouse Cochlea

Cochlear inner hair cells (IHCs) transmit acoustic signals to spiral ganglion neurons (SGNs) through ribbon synapses. Several experimental studies have indicated that hair cell synapses may be the initial targets in sensorineural hearing loss (SNHL). Such studies have proposed the concept of cochlear &#34;synaptopathy&#34;, which refers to alterations in ribbon synapse number, structure, or function that result in abnormal synaptic transmission between IHCs and SGNs. While cochlear synaptopathy is irreversible, it does not affect the hearing threshold. In noise-induced experimental models, restricted damage to IHC synapses in select frequency regions is employed to identify the environmental factors that specifically cause synaptopathy, as well as the physiological consequences of disturbing this inner ear circuit. Here, we present a protocol for analyzing cochlear synaptic morphology and function at a specific frequency region in adult mice. In this protocol, cochlear localization of specific frequency regions is performed using place-frequency maps in conjunction with cochleogram data, following which the morphological characteristics of ribbon synapses are evaluated via synaptic immunostaining. The functional status of ribbon synapses is then determined based on the amplitudes of auditory brainstem response (ABR) wave I. The present report demonstrates that this approach can be used to deepen our understanding of the pathogenesis and mechanisms of synaptic dysfunction in the cochlea, which may aid in the development of novel therapeutic interventions.

This manuscript describes an experimental protocol for evaluating the morphological characteristics and functional status of ribbon synapses in normal mice. The present model is also suitable for noise-induced and age-related cochlear synaptopathy-restricted models. The correlative results of previous mouse studies are also discussed.

Cochlear inner hair cells (IHCs) transmit acoustic signals to spiral ganglion neurons (SGNs) through ribbon synapses. Several experimental studies have ...

Cochlear Surface Preparation in the Adult Mouse

Auditory processing in the cochlea depends on the integrity of the mechanosensory hair cells. Over a lifetime, hearing loss can be acquired from numerous etiologies such as exposure to excessive noise, the use of ototoxic medications, bacterial or viral ear infections, head injuries, and the aging process. Loss of sensory hair cells is a common pathological feature of the varieties of acquired hearing loss. Additionally, the inner hair cell synapse can be damaged by mild insults. Therefore, surface preparations of cochlear epithelia, in combination with immunolabeling techniques and confocal imagery, are a very useful tool for the investigation of cochlear pathologies, including losses of ribbon synapses and sensory hair cells, changes in protein levels in hair cells and supporting cells, hair cell regeneration, and determination of report gene expression (i.e., GFP) for verification of successful transduction and identification of transduced cell types. The cochlea, a bony spiral-shaped structure in the inner ear, holds the auditory sensory end organ, the organ of Corti (OC). Sensory hair cells and surrounding supporting cells in the OC are contained in the cochlear duct and rest on the basilar membrane, organized in a tonotopic fashion with high-frequency detection occurring in the base and low-frequency in the apex. With the availability of molecular and genetic information and the ability to manipulate genes by knockout and knock-in techniques, mice have been widely used in biological research, including in hearing science. However, the adult mouse cochlea is miniscule, and the cochlear epithelium is encapsulated in a bony labyrinth, making microdissection difficult. Although dissection techniques have been developed and used in many laboratories, this modified microdissection method using cell and tissue adhesive is easier and more convenient. It can be used in all types of adult mouse cochleae following decalcification.

This article presents a modified cochlear surface preparation method that requires decalcification and use of a cell and tissue adhesive to adhere the pieces of cochlear epithelia to 10 mm round cover slips for immunohistochemistry in adult mouse cochleae.

Auditory processing in the cochlea depends on the integrity of the mechanosensory hair cells. Over a lifetime, hearing loss can be acquired from numerous ...

Dissection of the Endolymphatic Sac from Mice

The study of mutant mouse models of human hearing and balance disorders has unraveled many structural and functional changes which may contribute to the human phenotypes. Although important progress has been done in the understanding of the development and function of the neurosensory epithelia of the cochlea and vestibula, limited knowledge is available regarding the development, cellular composition, molecular pathways and functional characteristics of the endolymphatic sac. This is, in large part, due to the difficulty of visualizing and microdissecting this tissue, which is an epithelium comprised of only one cell layer. The study presented here describes an approach to access and microdissect the endolymphatic sac from the wild-type mouse inner ear at different ages. The result of a similar dissection is shown in a pendrin-deficient mouse model of enlargement of the vestibular aqueduct. A transgenic mouse with a fluorescent endolymphatic sac is presented. This reporter mouse can be used to readily visualize the endolymphatic sac with limited dissection and determine its size. It can also be used as an educational tool to teach how to dissect the endolymphatic sac. These dissection procedures should facilitate further characterization of this understudied part of the inner ear.

This study describes how to dissect the endolymphatic sac from the inner ear of the mouse at different ages. The result of a similar dissection is shown in an Slc26a4-null mouse model of enlargement of the endolymphatic sac. A transgenic mouse with a fluorescent reporter expressed in the endolymphatic sac is presented as a model to readily visualize the endolymphatic sac, and educational tool.

The study of mutant mouse models of human hearing and balance disorders has unraveled many structural and functional changes which may contribute to the ...

Stria Vascularis Microdissection for Single-Nucleus Sequencing or Immunostaining

Dissection of Adult Mouse Stria Vascularis for Single-Nucleus Sequencing or Immunostaining

Endocochlear potential, which is generated by the stria vascularis, is essential to maintain an environment conducive to appropriate hair cell mechanotransduction and ultimately hearing. Pathologies of the stria vascularis can result in a decreased hearing. Dissection of the adult stria vascularis allows for focused single-nucleus capture and subsequent single-nucleus sequencing and immunostaining. These techniques are used to study stria vascularis pathophysiology at the single-cell level. 
Single-nucleus sequencing can be used in the setting of transcriptional analysis of the stria vascularis. Meanwhile, immunostaining continues to be useful in identifying specific populations of cells. Both methods require proper stria vascularis dissection as a prerequisite, which can prove to be technically challenging.

Author Spotlight: Dissection of Adult Mouse Stria Vascularis for Single-Nucleus Sequencing or Immunostaining  

The stria vascularis is vital to the generation of endocochlear potential. Here, we present the dissection of the adult mouse stria vascularis for single-nucleus sequencing or immunostaining.