Immunocytochemical localization of carbonic anhydrase in the spinal cords of normal and mutant (shiverer) adult mice with comparisons among fixation methods

The peroxidase-antiperoxidase technique was used for immunocytochemical localization of carbonic anhydrase in the mouse spinal cord to detect whether this antigen was normally present in myelinated fibers, in oligodendrocytes in both white and gray matter, and in astrocytes, and to determine where the carbonic anhydrase might be localized in the spinal cords of dysmyelinating mutant (shiverer) mice. The most favorable methods for treating tissue were: 1) immersion in formalin-ethanol-acetic acid followed by paraffin embedding, or 2) light fixation with paraformaldehyde and preparation of vibratome sections. Carnoy's solution, followed by paraffin embedding, extracted myelin from the tissue, while aqueous aldehydes, when used before paraffin embedding, reduced staining everywhere except at sites of compact myelin. The latter conclusion was based, in part, on the almost complete loss of this antigen from the shiverer cord, where compact myelin is known to be virtually absent but where membrane-bound carbonic anhydrase was demonstrated enzymatically. When the optimal methods were used with normal mouse cords, carbonic anhydrase was found throughout the white matter columns and in the oligodendrocytes in gray and white matter. The staining of the white matter was attributed to myelinated fibers because of the similarity in distribution to both a histological myelin stain and the immunocytochemical staining for myelin basic protein. In the mutant mice the oligodendrocyte cell bodies and processes, which were stained in all areas of the spinal cord, were particularly numerous at the periphery of the sections. In contrast to the oligodendrocytes, the fibrous astrocytes appeared to lack carbonic anhydrase, or to have lower than detectable levels, since the astrocyte marker, glial fibrillary acidic protein, had a very different distribution from that of carbonic anhydrase. Even finer localization was obtained in vibratome sections, where the antibody against carbonic anhydrase permitted visualization of the processes connecting oligodendrocytes to myelinated fibers in the normal adult spinal cord.     

Complete penetration of antibodies into vibratome sections after glutaraldehyde fixation and ethanol treatment: light and electron microscopy for neuropeptides.

To develop a method for quantitative electron microscopic immunocytochemistry on neural tissue of CNS, we tested the extent to which ethanol treatment would improve the penetration of immunoreagents through vibratome sections fixed in high concentrations of glutaraldehyde without compromising ultrastructure. Transverse or sagittal vibratome sections (60-80 microns) of spinal cord perfused with 1% formaldehyde plus 1% or 2.5% glutaraldehyde were washed in 50% ethanol for 0-70 min and stained to reveal immunoreactivity for neuropeptide Y (NPY). Semi-thin (1 micron) or ultra-thin sections were used to assess the depth to which NPY nerve fibers in the dorsal horn were stained. Without ethanol washing, immunoreactive nerve fibers were visualized only in the surface 5-10 microns of transverse or sagittal vibratome sections. In transverse vibratome sections, NPY nerve fibers, which ran perpendicular to the cut surfaces of the sections, were entirely stained after a 30-min wash in 50% ethanol. The numbers of NPY-immunoreactive varicosities and synapses were comparable at the surfaces and in the centers of the vibratome sections. In sagittal sections, where NPY nerve fibers ran parallel to the cut surfaces, fibers in the centers of vibratome sections could not be labeled even after 70 min in 50% ethanol. Substance P- and enkephalin (Enk)-immunoreactive nerve fibers could also be completely stained in transverse sections of spinal cord or medulla oblongata after 30-min exposure to ethanol. Ethanol washing had no significant deleterious effects on ultrastructure, although the amount of cytoplasmic matrix in neurons decreased with increasing exposure. These results indicate that washing with 50% ethanol for at least 30 min allows immunoreagents to penetrate completely through nerve fibers fixed with high concentrations of glutaraldehyde, as long as the fibers have cut ends at both surfaces of a vibratome section. This technique makes possible quantitative electron microscopic immunocytochemical studies and is proving a useful tool for defining synaptic connections in the CNS.     

Histochemical Demonstration of Pyrophosphatase

Fresh tissue slices were fixed in 5% formalin containing 0.9% NaCl for 10-20 min and frozen sections therefrom floated for 3 hr at 37°C on an incubating mixture made as follows. Sodium pyrophosphate (Na₄P₂O₇-12H₂O), 1.088 gm was dissolved in 20-30 ml of distilled water and to this was added ferric chloride (FeCl₃-6H₂O), 0.61 gm dissolved in 10-15 ml of water. The precipitate was just dissolved by cautiously adding 5-10% aqueous Na₂CO₃ solution and the pH adjusted to 7.2 with 1N HCl. The volume was made up to 100 ml and 0.9 gm of NaCl added. Before use, 1 ml of 10% Mg(NO₃) was added. After incubation, sections were washed 10-15 min in 0.9% NaCl, then mounted on glass slides and air-dried. When dry, the slides were immersed in 0.9% NaCl containing 0.2-0.5% ammonium sulfide for 2-3 min, then dehydrated rapidly through graded alcohols, cleared, and covered in balsam. Sites of pyrophosphatase activity stained in various shades of green. Acid pyrophosphatase also was histochemically demonstrated by the same principle, excepting that the substrate solution was adjusted to pH 3.7-4.0 with acetate buffer. The pattern of distribution of pyrophosphatase and glycerophosphatase was almost identical.     

Staining of Oligodendroglia with Silver Ammino Tungstate in Unembedded and Embedded Material

Specimens of brain or spinal cord fixed in formalin, Cajal's formol-bromide, or Koenig, Groat and Windle's formalin-acacia can be used to stain oligodendrocytes in frozen, in paraffin, or in celloidin sections. The sections are soaked 3-5 min in 0.02% acetic acid, pH 3.4, then rinsed 2-3 sec in 3% H₂O₂ and transferred to a silver bath prepared as follows: Mix equal parts of 10% AgNO₃ and 10% Na₂WO₄, and dissolve the precipitate with concentrated NH₄OH; avoid an excess of ammonia. Silver at room temperature for 15-20 sec, develop in 1% formalin, dehydrate, and mount. For embedded material, prepare a mixture consisting of 1 part of 10% aqueous Aerosol MA and 4 parts of 10% Aerosol OT in 95% alcohol. Add 5 drops of this mixture to each 50 ml of dilute acetic acid and 3% H₂O₂; 5 drops to each 20 ml of the silver bath.     

On-The-Slide Impregnation by Albumen-OsO4, Selective for Ciliary Basal Bodies and Osmiophilic Granules in Synaptic Terminals

Procedure: Fix 24 hr by immersion in Heidenhain's Susa (2-4 mm specimens) or by perfusion for spinal cord or brain of cats or larger mammals. Wash in 80% alcohol containing 0.5% I₂, dehydrate, and embed in paraffin; or, better, double embed in celloidinparaffin. Attach sections to slides by albumen-glycerol. Remove paraffin, and celloidin if used, treat again with iodized alcohol for 30 min, followed by 0.25% Na₂S₂O₃, and wash well with distilled water. Impregnate in darkness for 5 days at 37 C in aqueous 0.66% OsO₄ to which 0.2% fresh egg albumen has been added. Check the impregnation microscopically and return the slide to the original staining solution for another 2-3 days if the granules do not show. Wash well in distilled water, dehydrate and cover as usual. The stain does not fade in water, alcohol or zylene; therefore almost any counterstain can be applied. The method stains selectively black the ciliary basal bodies and the osmiophilic granules in the majority of the different types of synaptic terminals; most red blood cells and a few nuclei also stain black.     

Improved Procedures in Fungal Cytology Utilizing Giemsa

To study nuclear events in fructifications of the Basidiomycetes, material was fixed 24 hr in a saturated aqueous solution of HgCl₂ containing 1% glacial acetic acid, and embedded in Aquax (G. T. Gurr Ltd.). Following a 4 hr hydrolysis at 20 C in 60% H₃PO₄, sections were stained for 30 min in a mixture of 4 ml Giemsa R66 (G T. Gurr Ltd.) and 100 ml phosphate buffer at pH 6.5. Differentiation was carried out in sodium cacodylate-HCl buffer at pH 5.8 when required. Preparations were dehydrated in an acetone-xylene series prior to mounting in Euparal. The use of paraffin wax as the embedding medium and HCl as the hydrolysing agent yielded preparations of an inferior quality.     

Hematoxylin-Eosin Staining of OsO4-Fixed Epon- Embedded Tissue; Prestaining Oxidation by Acidified H2O2

Successful application of hematoxylin-eosin staining to 0.5-1 μ sections of OsO₄-fixed Epon-embedded mammalian tissue is made possible by first treating the sections for approximately 1 min at 25-30 C with 10% H₂O₂ acidified with 0.1 or 0.01 N H₂SO₄ to pH 3.2. Subsequent steps are: washing; drying; Hams hematoxylin at 50 C, 1-2 min; washing; drying; 0.2-0.3% NH₄OH in 70% ethanol, 3-5 sec, drying at 50 C; 5% aqueous eosin for 3 & 45 sec at 25-30 C, washing; drying; clearing in xylene and mounting in resin. The use of acidified H₂O₂ prevents the staining of Epon and permits the characteristic staining picture to be obtained. Sections were attached to glass slides without adhesive and processed horizontally on a rack. Slides should be well drained and blotted before each drying step, to prevent formation of precipitate on the section.     

Silver Protein Staining of Nerve Fibers in Celloidin Sections

Celloidin sections from formalin-fixed brain and spinal cord of primates are stored in 70% alcohol after cutting, soaked in 2% pyridine in 50% alcohol for 6-8 hr at 37 C, and transferred to 1% concentrated NH₄OH in 50% alcohol 15-18 hr at 20-25 C. After washing and flattening, the sections are transferred to 1% silver protein solution containing 30 ml of 0.2 M H₃BO₃/100 ml. Impregnation is accomplished in 50 ml screw-top jars, 50 mm in diameter, which are filled to a depth of 35 mm, and have 1 gm of copper foil, 0.002 inch thick added. The foil is folded in loose accordion-fashion, pierced and threaded, cleaned in 5% HNO₃, rinsed in distilled water, and suspended in the solution just above the sections by fastening the thread to the jar lid. The sections are impregnated for 24 hr at 37 C, rinsed in distilled water, reduced in a solution of 5% Na₂SO₃ and 1% hydroquinone for 10 min, washed in distilled water and toned in 0.2% gold chloride for 5 min. After rinsing in distilled water, the sections are transferred to 1% oxalic acid for 45-60 sec, washed in distilled water and placed in 5% Na₂S₂O₃ for 5 min. Sections are then washed, dehydrated to 95% alcohol, cleared in terpineol, followed by 3 changes in xylene, and mounted.     

Nile Blue Histochemical Method for Phospholipids

The technic recommended is: Fix 6-12 hr. in 10% formalin containing 1% CaCl₂. Cut frozen sections without embedding or after gelatin or carbowax. Stain 90 min. at 60°C. in saturated aqueous Nile blue sulfate, 500 ml. plus 50 ml. of 0.5% H₂SO₄, boiled 2 hr. before use. Rinse in distilled water, and place in acetone heated to 50°C. Remove the acetone from the source of heat and allow the sections to remain 30 min. Differentiate in 5% acetic acid 30 min., rinse in distilled water, and refine the differentiation in 0.5% HCl for 3 min. Wash in several changes of distilled water and mount in glycerol jelly. Results: phospholipids - blue; everything else - unstained. Counterstaining nuclei with safranin is optional, but if done, it preferably precedes the Nile blue and is then differentiated by the acetic acid. The histochemical principles on which the method is based are as follows: (1) The calcium compounds of phospholipids combine with the oxazine form of Nile blue sulfate and survive subsequent treatment; (2) neutral lipids are dissolved out by acetone; (3) proteins and other interfering substances are destained by the acetic acid and hydrochloric acid baths.     

Fixation and embedding variables in the immuno-electron microscopic study of rat heymann nephritis

Summary Fixation and embedding variables were compared in immuno-electron microscopic localization of rat IgG in an autologous immune complextype nephritis. Specimens from kidney cortex were fixed for 3, 6 or 9 h in the following fixatives made in 0.1 M phosphate buffer at pH 7.44% paraformaldehyde, 2.5% glutaraldehyde, periodate-lysine-paraformaldehyde or modified Karnovsky's fixative. Localization of IgG was performed on tissue sections cut with a tissue chopper, cryostat or sliding microtome, using agarose, Ames O.C.T. Compound or polyethylene glycol respectively as cutting matrixes. The sections were incubated in peroxidase-labelled antirat IgG antiserum (diluted 120 with phosphate-buffered saline) for 60 h. Peroxidase activity was then revealed and the sections embedded in Epon. Exact localization of IgG throughout the sections and good ultrastructure were achieved when paraformaldehyde and agarose were used. Periodate-lysine-paraformaldehyde proved almost as useful as paraformaldehyde in connection with agarose in respect of peroxidase reaction and ultrastructure. Fixatives containing glutaraldehyde gave a mostly weak and unevenly distributed peroxidase reaction product. In the cryostat sections breaking of the tissue structure could not be avoided. When polyethylene glycol was used as cutting matrix no peroxidase reaction was achieved.     

Agarose Gel Electrophoresis for the Separation of DNA Fragments

Agarose gel electrophoresis is the most effective way of separating DNA fragments of varying sizes ranging from 100 bp to 25 kb¹. Agarose is isolated from the seaweed genera Gelidium and Gracilaria, and consists of repeated agarobiose (L- and D-galactose) subunits². During gelation, agarose polymers associate non-covalently and form a network of bundles whose pore sizes determine a gel''s molecular sieving properties. The use of agarose gel electrophoresis revolutionized the separation of DNA. Prior to the adoption of agarose gels, DNA was primarily separated using sucrose density gradient centrifugation, which only provided an approximation of size. To separate DNA using agarose gel electrophoresis, the DNA is loaded into pre-cast wells in the gel and a current applied. The phosphate backbone of the DNA (and RNA) molecule is negatively charged, therefore when placed in an electric field, DNA fragments will migrate to the positively charged anode. Because DNA has a uniform mass/charge ratio, DNA molecules are separated by size within an agarose gel in a pattern such that the distance traveled is inversely proportional to the log of its molecular weight³. The leading model for DNA movement through an agarose gel is "biased reptation", whereby the leading edge moves forward and pulls the rest of the molecule along⁴. The rate of migration of a DNA molecule through a gel is determined by the following: 1) size of DNA molecule; 2) agarose concentration; 3) DNA conformation⁵; 4) voltage applied, 5) presence of ethidium bromide, 6) type of agarose and 7) electrophoresis buffer. After separation, the DNA molecules can be visualized under uv light after staining with an appropriate dye. By following this protocol, students should be able to: 1. Understand the mechanism by which DNA fragments are separated within a gel matrix 2. Understand how conformation of the DNA molecule will determine its mobility through a gel matrix 3. Identify an agarose solution of appropriate concentration for their needs 4. Prepare an agarose gel for electrophoresis of DNA samples 5. Set up the gel electrophoresis apparatus and power supply 6. Select an appropriate voltage for the separation of DNA fragments 7. Understand the mechanism by which ethidium bromide allows for the visualization of DNA bands 8. Determine the sizes of separated DNA fragments       

Prestaining Oxidation by Acidified H2O2 for Revealing Schiff-Positive Sites in Epon-Embedded Sections

Reliable production and identification of Schiff-positive sites on glutaraldehyde-osmium fixed 0.5-1 μsm Epon sections is accomplished by preoxidation of sections with 10% H₂O₂ acidified with H₂SO₄ (HPSA) to pH 3.2 (Pool, C. R., Stain Techn., 44: 75-9, 1969). Light green as a counterstain is used. Steps in the procedure are: HPSA, 1-2 min at 25-30 C; washing; 1% light green 3-5 min; brief rinse; Schiff reagent 1-3 min; washing; drying; clearing in xylene and mounting in resin. The use of acidified H₂O₂ prevents the common occurrence of Schiff background staining in glutaraldehyde-fixed tissues and permits optimum penetration of staining solutions. Sections were attached to glass slides without adhesive and were processed in Coplin jars. Prior to drying, excess solutions should be drained and wiped away with lens tissue to prevent formation of precipitate on the sections.     

Characterization, Distribution, and Protein Kinase C-Mediated Regulation of [35S]Glutathione Binding Sites in Mouse and Human Spinal Cord

Abstract: We have characterized a high-affinity [³⁵S]-glutathione ([³⁵S]GSH) binding site in mouse and human spinal cord. [³⁵S]GSH binding sites in mouse and human spinal cord were observed largely within the gray matter in both the dorsal and ventral horns of spinal cord at cervical, thoracic, and lumbosacral segments. High-affinity [³⁵S]GSH binding was saturable, showing a B _max of 72 fmol/mg of protein and a K _D of 3.0 n M for mouse spinal cord and a B _max of 52 fmol/mg of protein and a K _D of 1.6 n M for human spinal cord. [³⁵S]GSH binding was displaceable by GSH, l -cysteine, and S -hexyl-GSH, but not by glutamate, glycine, or NMDA. These [³⁵S]GSH binding sites exhibited kinetic and saturation characteristics similar to GSH binding sites in rat brain astrocytes. To determine whether [³⁵S]GSH binding sites could be regulated by protein kinase C, we exposed human spinal cord sections to phorbol 12,13-diacetate for 1 h before ligand binding. Phorbol ester treatment increased [³⁵S]GSH binding by ∼60%, an effect that could be blocked by exposure of spinal cord sections to 1-(5-isoquinolinylsulfonyl)-2-methylpiperazine, a general protein kinase inhibitor. [³⁵S]GSH binding sites in the spinal cord of both species exhibited many of the characteristics of a receptor including saturable binding, high affinity, ligand specificity, and modulation by kinase activity. These data suggest that GSH is a neurotransmitter in the CNS.     

Enkephalin, substance P, and serotonin axonal input to c-fos-like immunoreactive neurons of the rat spinal cord

Mustard oil, which stimulates small diameter afferents, was used to evoke the expression of the oncogene c-fos in the lumbar spinal cord. C-fos-like immunoreactivity was concentrated in, but not limited to, neuronal nuclei of laminae I and II of the lumbar dorsal horn. Double-label immunocytochemistry was used to determine if neurons which expressed c-fos-like immunoreactivity received axonal input from enkephalin-, substance P- or serotonin-immunoreactive neurons. The analysis of vibratome and semithin plastic-embedded tissue sections demonstrated that the majority of c-fos-like immunoreactive neurons received input from enkephalin-, substance P- or serotonin-immunoreactive axonal varicosities.     

Proteome analysis of up-regulated proteins in the rat spinal cord induced by transection injury

The inability of the CNS to regenerate in adult mammals propels us to reveal associated proteins involved in the injured CNS. In this paper, either thoracic laminectomy (as sham control) or thoracic spinal cord transection was performed on male adult rats. Five days after surgery, the whole spinal cord tissue was dissected and fractionated into water-soluble (dissolved in Tris buffer) and water-insoluble (dissolved in a solution containing chaotropes and surfactants) portions for 2-DE. Protein identification was performed by MS and further confirmed by Western blot. As a result, over 30 protein spots in the injured spinal cord were shown to be up-regulated no less than 1.5-fold. These identified proteins possibly play various roles during the injury and repair process and may be functionally categorized as several different groups, such as stress-responsive and metabolic changes, lipid and protein degeneration, neural survival and regeneration. In particular, over-expression of 11-zinc finger protein and glypican may be responsible for the inhibition of axonal growth and regeneration. Moreover, three unknown proteins with novel sequences were found to be up-regulated by spinal cord injury. Further characterization of these molecules may help us come closer to understanding the mechanisms that underlie the inability of the adult CNS to regenerate.     

Autoradiographic distribution of I-galanin binding sites in the rat central nervous system

Galanin (GAL) binding sites in coronal sections of the rat brain were demonstrated using autoradiographic methods. Scatchard analysis of ¹²⁵I-GAL binding to slide-mounted tissue sections revealed saturable binding to a single class of receptors with a Kd of approximately 0.2 nM. ¹²⁵I-GAL binding sites were demonstrated throughout the rat central nervous system. Dense binding was observed in the following areas: prefrontal cortex, the anterior nuclei of the olfactory bulb, several nuclei of the amygdaloid complex, the dorsal septal area, dorsal bed nucleus of the stria terminalis, the ventral pallidum, the internal medullary laminae of the thalamus, medial pretectal nucleus, nucleus of the medial optic tract, borderline area of the caudal spinal trigeminal nucleus adjacent to the spinal trigeminal tract, the substantia gelatinosa and the superficial layers of the dorsal spinal cord. Moderate binding was observed in the piriform, periamygdaloid, entorhinal, insular cortex and the subiculum, the nucleus accumbens, medial forebrain bundle, anterior hypothalamic, ventromedial, dorsal premamillary, lateral and periventricular thalamic nuclei, the subzona incerta, Forel's field H₁ and H₂, periventricular gray matter, medial and superficial gray strata of the superior colliculus, dorsal parts of the central gray, peripeduncular area, the interpeduncular nucleus, substantia nigra zona compacta, ventral tegmental area, the dorsal and ventral parabrachial and parvocellular reticular nuclei. The preponderance of GAL-binding in somatosensory as well as in limbic areas suggests a possible involvement of GAL in a variety of brain functions.     

Assessing Neural Stem Cell Motility Using an Agarose Gel-based Microfluidic Device

While microfluidic technology is reaching a new level of maturity for macromolecular assays, cell-based assays are still at an infant stage¹. This is largely due to the difficulty with which one can create a cell-compatible and steady microenvironment using conventional microfabrication techniques and materials. We address this problem via the introduction of a novel microfabrication material, agarose gel, as the base material for the microfluidic device. Agarose gel is highly malleable, and permeable to gas and nutrients necessary for cell survival, and thus an ideal material for cell-based assays. We have shown previously that agarose gel based devices have been successful in studying bacterial and neutrophil cell migration². In this report, three parallel microfluidic channels are patterned in an agarose gel membrane of about 1mm thickness. Constant flows with media/buffer are maintained in the two side channels using a peristaltic pump. Cells are maintained in the center channel for observation. Since the nutrients and chemicals in the side channels are constantly diffusing from the side to center channel, the chemical environment of the center channel is easily controlled via the flow along the side channels. Using this device, we demonstrate that the movement of neural stem cells can be monitored optically with ease under various chemical conditions, and the experimental results show that the over expression of epidermal growth factor receptors (EGFR) enhances the motility of neural stem cells. Motility of neural stem cells is an important biomarker for assessing cells aggressiveness, thus tumorigenic factor³. Deciphering the mechanism underlying NSC motility will yield insight into both disorders of neural development and into brain cancer stem cell invasion.Download video file.^{(81M, mov)}     

Cytochemical observations on mannose-specific binding sites for horseradish peroxidase in liver sinusoidal cells

Paraformaldehyde-fixed, frozen sections of the liver of rats were processed for the detection of mannose-specific binding sites of horseradish peroxidase (HRP) by a method reported previously, with some modifications resulting in a more intense binding reaction. Before staining for peroxidase activity, the sections were held in buffered solutions of physiological saline at different temperatures and pH's, and in the presence or absence of added Ca2+, mannose or galactose. The gradual decrease and final disappearance of the binding reaction were observed. The release of HRP from the binding sites as determined by the disappearance of the cytochemical reaction was 50-100 times faster at 22 degrees C than at 4 degrees C and was 5-10 times faster at 37 degrees C than at 22 degrees C. The release was approximately twice as fast at pH 7.0 than at pH 9.0 and 20-30 times faster at pH 6.0 than at pH 7.0. The release of HRP was 10-15 times faster in the absence of 1 mM Ca2+ in the buffer solution and was approximately 100 times faster in the presence of 0.1 M D-mannose as compared to 0.1 M D-galactose. Pretreatment of the sections with trypsin abolished the binding reaction whereas neuraminidase, phospholipases A2 and C, and chondroitinase ABC were without effect. An acidic isoenzyme of HRP, Sigma type VIII, was bound more intensely and more widely to liver sinusoidal cells than another acidic isoenzyme, Sigma type VII, a basic isoenzyme, Sigma type IX, and the routinely used preparation, Sigma type VI. The effect of the temperature on the binding reaction was re-examined with an improved procedure. In contradistinction to the previous finding, strong binding of HRP after 2-4 h incubation at 4 degrees C was observed.     

Differentiated Staining of Osmium Tetroxide-Fixed, Vestopal-w-Embedded Tissue in thin Sections

Tissues were fixed at 20° C for 1 hr in 1% OsO₄, buffered at pH 7.4 with veronal-acetate (Palade's fixative), soaked 5 min in the same buffer without OsO₄, then dehydrated in buffer-acetone mixtures of 30, 50, 75 and 90% acetone content, and finally in anhydrous acetone. Infiltration was accomplished through Vestopal-W-acetone mixtures of 1:3, 1:1, 3:1 to undiluted Vestopal. After polymerisation at 60° C for 24 hr, 1-2 μ sections were cut, dried on slides without adhesive, and stained by any of the following methods. (1) Mayer's acid hemalum: Flood the slides with the staining solution and allow to stand at 20°C for 2-3 hr while the water of the solution evaporates; wash in distilled water, 2 min; differentiate in 1% HCl; rinse 1-2 sec in 10% NH,OH. (2) Iron-trioxyhematein (of Hansen): Apply the staining solution as in method 1; wash 3-5 min in 5% acetic acid; restain for 1-12 hr by flooding with a mixture consisting of staining solution, 2 parts, and 1 part of a 1:1 mixture of 2% acetic acid and 2% H₂SO₄ (observe under microscope for staining intensity); wash 2 min in distilled water and 1 hr in tap water. (3) Iron-hematoxylin (Heidenhain): Mordant 6 hr in 2.5% iron-alum solution; wash 1 min in distilled water; stain in 1% or 0.5% ripened hematoxylin for 3-12 br; differentiate 8 min in 2.5%, and 15 min in 1% iron-alum solution; wash 1 hr in tap water. (4) Aceto-carmine (Schneider): Stain 12-24 hr; wash 0.5-1.0 min in distilled water. (5) Picrofuchsin: Stain 24-48 hr in 1% acid fuchsin dissolved in saturated aqueous picric acid; differentiate for only 1-2 sec in 96% ethanol. (6) Modified Giemsa: Mix 640 ml of a solution of 9.08 gm KH₂PO₄ in 1000 ml of distilled water and 360 ml of a solution of 11.88 gm Na₂HPO₄-2H₂O in 1000 ml of distilled water. Soak sections in this buffer, 12 hr. Dissolve 1.0 gm of azur I in 125 ml of boiling distilled water; add 0.5 gm of methylene blue; filter and add hot distilled water until a volume of 250 ml is reached (solution “AM”). Dissolve 1.5 gm of eosin, yellowish, in 250 ml of hot distilled water; filter (solution “E”). Mix 1.5 ml of “AM” in 100 ml of buffer with 3 ml of “E” in 100 ml of buffer. Stain 12-24 hr. Differentiate 3 sec in 25 ml methyl benzoate in 75 ml dioxane; 3 sec in 35 ml methyl benzoate in 65 ml acetone; 3 sec in 30 ml acetone in 70 ml methyl benzoate; and 3 sec in 5 ml acetone in 95 ml methyl benzoate. Dehydrated sections may be covered in a neutral synthetic resin (Caedax was used).