Aceto-Carmine-Lactophenol Preparations Of Paramecium Aurelia

Paramecia were killed and stained by adding a sat. soln. of carmine in acetic acid to a small drop of culture, cleared with 45% acetic acid as soon as the nuclei became darkly colored, and mounted in lactophenol (phenol crystals, 20 g.; lactic acid, 20 ml.; glycerol, 40 ml.; distilled water, 20 ml.). The mounting mixture was prepared by warming to dissolve the phenol and 20 drops of aceto-carmine added after cooling. Cover glasses were ringed with colorless nail polish or with asphaltum after slides had stood several days.     

Selective Silver Impregnation of Degenerating Axons In The Central Nervous System

Rat and rabbit brains containing surgical lesions of 5-10 days' duration were fixed in 10% formalin (neutralized with calcium carbonate) for 1 week to 6 months. Frozen sections (15-20 n) were rinsed and then soaked 7 minutes in a 1.7% solution of strong ammonia in distilled water. Subsequent treatment was as follows: rinse; 0.05% aqueous potassium permanganate 5-15 minutes; 0.5% aqueous potassium metabisulfite, 2 changes of 2.5 minutes each; wash thoroughly in 3 changes distilled water; 1.5% aqueous silver nitrate, 0.5-1.0 hr.; 1% citric acid, 5-10 sec.; 2 changes distilled water; 1% sodium thiosulfate, 30 see.; 3 changes distilled water. Each section is then processed separately. Ammoniacal silver solution (450 mg. silver nitrate in 10 ml. distilled water; add 5 ml. ethanol; let cool to room temperature; add 1 ml. strong ammonia water and 0.9 ml. of 2.5% aqueous sodium hydroxide), 0.5-1.0 min. with gentle agitation. Reduction of about 1 minute is accomplished in: distilled water, 45 ml.; ethanol, 5 ml.; 10% formalin, 1.5 ml.; 1% citric acid, 1.5 ml. Rinsing; 1% sodium thiosulfate, 10 sec.; thorough washing followed by dehydration through graded alcohol and 3 changes of xylene or toluene complete the staining process. Normal nerve fibers are slightly stained to unstained, degenerating fibers, black. The treatment in potassium permanganate is critical since too little favors overstaining of normal fibers and too much abolishes staining of degenerating fibers.     

A Protargol Method for Staining Nerve Fibers in Frozen or Celloidin Sections

Extensive experimentation with protargol staining of neurons in celloidin and frozen sections of organs has resulted in the following technic: Fix tissue in 10% aqueous formalin. Cut celloidin sections IS to 25 μ, frozen sections 25 to 40 μ. Place sections for 24 hours in 50% alcohol to which 1% by volume of NH₄OH has been added. Transfer the sections directly into a 1% aqueous solution of protargol, containing 0.2 to 0.3 g. of electrolytic copper foil which has been coated with a 0.5% solution of celloidin, and allow to stand for 6 to 8 hours at 37° C. Caution: In this and the succeeding step the sections must not be allowed to come in contact with the copper. From aqueous protargol, place the sections for 24 to 48 hours at 37° C. directly into a pyridinated solution of alcoholic protargol (1.0% aqueous solution protargol, 50 ml.; 95% alcohol, 50 ml.; pyridine, 0.5 to 2.0 ml.), containing 0.2 to 0.3 g. of coated copper. Rinse briefly in 50% alcohol and reduce 10 min. in an alkaline hydroquinone reducer (H₃BO₃, 1.4 g.; Na₂SO₃, anhydrous, 2.0 g.; hydroquinone, 0.3 g.; distilled water, 85 cc; acetone, 15 ml.). Wash thoroly in water and tone for 10 min. in 0.2% aqueous gold chloride, acidified with acetic acid. Wash in distilled water and reduce for 1 to 3 min. in 2% aqueous oxalic acid. Quickly rinse in distilled water and treat the sections 3 to 5 min. with 5% aqueous Na₂S₂O₃+5H₂O. Wash in water and stain overnight in Einarson's gallocyanin. Wash thoroly in water and place in 5% aqueous phosphotungstic acid for 30 min. From phosphotungstic acid transfer directly to a dilution (stock solution, 20 ml.; distilled water, 30 ml.) of the following stock staining solution: anilin blue, 0.01 g.; fast green FCF, 0.5 g.; orange G, 2.0 g.; distilled water, 92.0 ml.; glacial acetic acid, 8 ml.) and stain for 1 hour. Differentiate with 70% and 95% alcohol; pass the sections thru butyl alcohol and cedar oil; mount.     

Silver Impregnation of Degenerating Axons in the Central Nervous System: A Modified Technic

Frozen sections of formalin-fixed brains containing surgical lesions, were treated with 15% ethanol for 0.5 hr., soaked in 0.5% phosphomolybdic acid for 0.25-1.0 hr., and subsequently treated with 0.05% potassium permanganate for 4-10 min. (The duration of the latter treatment is critical and individually variable). Subsequent procedure is as follows: decolorize in a mixture of equal parts of 1% hydroquinone and 1% oxalic acid; wash thoroughly and soak sections in 1.5% silver nitrate for 20-30 min.; ammoniacal silver nitrate (silver nitrate 0.9 g., distilled water 20 ml., pure ethanol 10 ml., strong ammonia 1.8 ml., 2.5% sodium hydroxide 1.5 ml.) 0.5-1.0 min.; reduce in acidified formalin (distilled water 400 ml., pure ethanol 45 ml., 1% citric acid 13.5 ml., 10% formalin 13.5 ml.) 1 min.; wash, and pass section through 1 % sodium thiosulf ate (0.5-1.0 min.); wash thoroughly and pass sections through graded alcohols and xylene (3 changes); cover in neutral synthetic resin.     

Modification of the Marchi Technic

The formula proposed by Swank and Davenport (1935) was modified and applied to human and macaque nervous material. Three groups of experiments were performed and the following observations were made. (1) Diluting the osmic acid component, without altering the relative concentration of the other constituents of the solution resulted in practically no staining of the degenerated fibers. (2) When all constituents of the staining solution were used in much lower concentration than previously suggested, enhancement of staining of the degenerating fibers occurred and the different structures of the normal tissue were more easily identified. (3) At low concentrations of osmic acid and potassium chlorate, the contrast was diminished and artifacts produced by increasing the concentration of acetic acid or formalin or both. The new formula, based on the present results, consists of osmic acid, 0.5%, 11 ml.; potassium chlorate, 1%, 16 ml.; formalin (cone), 3 ml.; acetic acid, 10%, 3 ml.; and distilled water to make 100 ml. (All solutions are aqueous). Good staining after a long period of fixation in formalin, following degeneration of 8-80 days, was obtained and the cost of staining solution greatly reduced.     

In vitro degradation of cell-wall and digestibility of cereal straws treated with anaerobic ruminal fungi

Ruminal fungal isolates (Orpinomyces sp.; C-14, Piromyces sp.; C-15, Orpinomyces sp.; B-13 and Anaeromyces sp.; B-6), were evaluated under anoxic conditions for their effect on in vitro dry matter digestibility, neutral detergent fibre, acid detergent fibre and acid detergent lignin using rice and wheat straw as substrate. There was no significant effect of the fungal isolates on the disappearance of the substrates along with rumen liquor when compared to control. The doses of 10(6) cfu/ml of the isolate were found to have maximum degradation of straws in comparison to the doses of 10(3) cfu/ml.     

A Single solution iron-hematoxylin Stain for Intestinal Protozoa

A single solution iron-hematoxylin stain is described for staining fecal smears rapidly and simply. The stain is prepared from the following solutions: Solution A: 1% hematoxylin in 95% alcohol, prepared by diluting a stock solution of 10% hematoxylin in 95% alcohol. Solution B: Ferric ammonium sulfate (violet crystals), 4.0 g.; glacial acetic acid, 1.0 ml.; concentrated sulfuric acid (sp. gr. 1.8),0.12 ml.; distilled water, 100 ml. Mix equal parts of Solution A and Solution B; allow to stand overnight, filter and use. For maximum length of staining life, store in full, air-tight bottles. To stain fecal smears, fix in Schaudinn's, pass through iodine alcohol to 50% alcohol, stain for three minutes, wash in running tap water 5 to 15 minutes, dehydrate and mount.     

A Single solution iron-hematoxylin Stain for Intestinal Protozoa

A single solution iron-hematoxylin stain is described for staining fecal smears rapidly and simply. The stain is prepared from the following solutions: Solution A: 1% hematoxylin in 95% alcohol, prepared by diluting a stock solution of 10% hematoxylin in 95% alcohol. Solution B: Ferric ammonium sulfate (violet crystals), 4.0 g.; glacial acetic acid, 1.0 ml.; concentrated sulfuric acid (sp. gr. 1.8),0.12 ml.; distilled water, 100 ml. Mix equal parts of Solution A and Solution B; allow to stand overnight, filter and use. For maximum length of staining life, store in full, air-tight bottles. To stain fecal smears, fix in Schaudinn's, pass through iodine alcohol to 50% alcohol, stain for three minutes, wash in running tap water 5 to 15 minutes, dehydrate and mount.     

A Chrome-Alum Preparation for Delicate and Difficult Fixations

A chrome-alum fixative is recommended as a reagent for general use. The basic formula is: C.P. chrome-alum, 3 g.; 40% formaldehyde, 30 ml.; glacial acetic acid, 2 ml.; distilled water, 238 ml. This fixative permits easy sectioning of yolk-rich amphibian embryos. It can be used to make permanent slides of Euglena showing the flagellum. It is a satisfactory fixative for insect larvae and fixes sharply the slime droplets of Planarians. Fixation should not exceed two hours or the material being fixed will swell. Rinses of 70% alcohol or water may follow the fluid. The fluid keeps well, does not harden tissues and gives good cytological detail.     

THE ENUMERATION OF LACTOBACILLI ON GRASS AND IN SILAGE

SUMMARY: For the enumeration of lactobacilli on grass and in silage the following medium has shown promise: peptone, meat extract and glucose, 10 g. each; tomato extract, 200 ml.; yeast autolysate, 50 ml.; Tween 80, 0.5 ml.; agar, 15 g., in a final volume of 1 1. and containing acetic acid/sodium acetate buffer in 0.2M concentration; pH 5–4. The medium was adjusted to pH 5–4 before sterilization and the requisite amount of concentrated pH 5.4 acetate buffer added just before plating. Double laver plates were used.
The only other silage organisms which in this medium formed colonies comparable in size with those of lactobacilli were heterofermentative streptococci and a micrococcus.     

Staining Sections of Peripheral Nerves for Axis Cylinders and for Myelin Sheaths

Pieces of mammalian nerves 1 to 2 cm. long were placed under moderate tension and fixed 24-48 hours in: picric acid, saturated aqueous, 90 ml.; formalin, 10 ml.; and trichloracetic acid, 25% aqueous, 2 ml. They were washed in water, cut in two and one end stained with 0.04-0.06% osmic acid solution, while the other was dehydrated, embedded in paraffin, and mounted sections from it stained with protargol. The fixing solution used was selected from a number of combinations of acidified picro-formalin as the one most likely to give satisfactory results when followed by both silver and osmic acid. The use of osmic acid solutions of less than 0.1% concentration avoided the overstaining of myelin sheaths seen frequently when stronger solutions were used with material that had been fixed previously. Protargol, 0.5% solution with fast green FCF added to make 0.05% dye in the final concentration, was used to impregnate sections for axis cylinders. Reduction and toning were done as in Bodian's method.     

Staining Sections of Peripheral Nerves for Axis Cylinders and for Myelin Sheaths

Pieces of mammalian nerves 1 to 2 cm. long were placed under moderate tension and fixed 24–48 hours in: picric acid, saturated aqueous, 90 ml.; formalin, 10 ml.; and trichloracetic acid, 25% aqueous, 2 ml. They were washed in water, cut in two and one end stained with 0.04–0.06% osmic acid solution, while the other was dehydrated, embedded in paraffin, and mounted sections from it stained with protargol. The fixing solution used was selected from a number of combinations of acidified picro-formalin as the one most likely to give satisfactory results when followed by both silver and osmic acid. The use of osmic acid solutions of less than 0.1% concentration avoided the overstaining of myelin sheaths seen frequently when stronger solutions were used with material that had been fixed previously. Protargol, 0.5% solution with fast green FCF added to make 0.05% dye in the final concentration, was used to impregnate sections for axis cylinders. Reduction and toning were done as in Bodian's method.     

Staining of Nerve Fibers with Methylene Blue Factors Improving the Staining

Several factors influencing the staining of nerve fibers with methylene blue, especially the influence of chloralhydrate and carbamylcholine chloride (as parasympathicotonics), and of some anesthetics were studied. The intestines of mouse, rat, and guinea pig were used. The following immersion technic is suggested: Tissue from animals anesthetised by chloralhydrate is immersed in: zinc free methylene blue, 0.03%; sodium tartrate, 0.5%; sodium pyruvate, 0.05% carbamylcholine, 0.00005%; 0.2 M Na₂HPO₄, 0.77%; 0.1 M citric acid, 0.18%; NACl, 0.79%; also an anesthetic which varies with the animal selected. Air is kept bubbling through the staining solution and microscopic examination is made at 6 min. intervals. After 0.5-1 hr. the tissue is fixed in: ammonium molyb-date, 10 g.; sucrose, 35 g.; distilled water, 100 ml.; to which is added just before use, 1% platinum chloride, 3 ml.; 2% osmic acid, 3 drops. Washing is in ice cold water and dehydration at 0°C. in Lang's fluids (varying mixtures of ethanol and n-butanol). The tissues thus prepared are stored in liquid paraffin.     

An Improved Gelatin Adhesive for Paraffin Sections

A two-solution adhesive, shown to keep for over two years at room temperature, consists of the following: (A) gelatin, 1 g.; calcium propionate, 1 g.; Roccal (10% benzalkonium chloride), 1 ml.; water, 100 ml.: (B) chrome alum (cryst.), 1 g.; water, 90 ml.; formalin, 10 ml. For flooding slides, mix 1 volume of A with 9 of B. Remove excess by blotting and wiping around the edges of sections. The adhesive is suitable for hard-to-affix material.     

A Simple Histochemical Reaction for Aldehydes

A study has been made on the possibility of replacing leucofuchsin by colored basic fuchsin for the histochemical demonstration of aldehydes. Several tissues from mammals and various pertinent fixatives were used. Aldehydes were freed from carbohydrates by oxidation and from thymonucleic acid by hydrolysis.

It was found that the colored form and not necessarily the leucoform of basic fuchsin can be used histochemically in demonstrating aldehydes. The technic used is as follows: (1) Treat with 1.0-0.5% H₅IO₆ (or in 1% KIO₄ in M/1 H₂SO₄) for 5 to 10 min. and wash thoroughly. For thymonucleic acid hydrolize with N HCl 5 min. at room temperature, 10 min. at 60°C. and 5 min. at room temperature. (2) Stain for 2-3 min. with 0.05% basic fuchsin in 5% ethanol, 3% phenol. (3). Transfer immediately to 1 or 2 changes of 1% sodium bisulphite or potassium metabisulphite in 0.1-0.2 N H₂SO₄ for a total of 5 min. (4) Rinse with water and treat with M H₂SO₄ in 95% ethanol for 3-5 min. 6. Wash thoroughly in water and dehydrate, clear, and mount. For glycogen and mucin the following counterstaining solution is recommended: orange G, 0.25 g.; light green SFY, 0.10 g.; phosphotungstic acid 0.50 g.; 50% ethanol, 100 ml.; glacial acetic acid, 0.25 ml.     

A Rapid Bulk Nissl Method

A simplified and time-saving Nissl method is described in which the fresh nervous tissue is placed directly into: dioxane, 65-70 ml.; water, 15 ml.; 95% alcohol, 20-15 ml.; and toluidine blue, 1 g. This solution fixes, stains, partially clears, and dehydrates in one procedure. The material is then sectioned according to a dry-ice method and mounted on the slide either with or without the use of the rapid albumen procedure. Thus it is possible to terminate an experiment one day and have the tissue ready for microscopic observation on the next.     

Differential Staining of Gastric Glandular Cells

Fundus of stomach is fixed in 10% formalin (aqueous), Bouin's fluid or 5% trichloracetic acid (aqueous). It is embedded in paraffin, and 7μ sections are cut, mounted, deparaffinized and passed to 70% alcohol and then stained as follows: Mordant 3 min. in saturated Bismarck brown in 70% alcohol. Rinse in 70% alcohol, pass to distilled water, then overstain (2 hr.) in aniline blue, 0.5% solution in 2.5% acetic acid (aqueous). Precipitate the anilin blue with 0.5 ml. of 0.1% methyl violet solution (aqueous) dropped on die slide. Leave on 2 min. or less. Wash and differentiate in 70% alcohol. (Parietal cells dark blue). Stain 30 min. in a mixture of hematein, 0.10g.; A1C13 cryst., 0.05g.; and 70% alcohol 50 ml., prepared just before use and not filtered. Rinse in 70% alcohol and differentiate with an alcoholic extract of saffron (2 g. saffron pistils in 100 ml. 90% alcohol at 60°C. for 6 hr.) while observing the progress of differentiation microscopically. Dehydrate by dropping a 0.1 % solution of acetic acid in absolute alcohol on the section for 30 sec., followed by pure absolute alcohol, xylene, and covering in balsam.     

Differential Staining of Gastric Glandular Cells

Fundus of stomach is fixed in 10% formalin (aqueous), Bouin's fluid or 5% trichloracetic acid (aqueous). It is embedded in paraffin, and 7μ sections are cut, mounted, deparaffinized and passed to 70% alcohol and then stained as follows: Mordant 3 min. in saturated Bismarck brown in 70% alcohol. Rinse in 70% alcohol, pass to distilled water, then overstain (2 hr.) in aniline blue, 0.5% solution in 2.5% acetic acid (aqueous). Precipitate the anilin blue with 0.5 ml. of 0.1% methyl violet solution (aqueous) dropped on die slide. Leave on 2 min. or less. Wash and differentiate in 70% alcohol. (Parietal cells dark blue). Stain 30 min. in a mixture of hematein, 0.10g.; A1C13 cryst., 0.05g.; and 70% alcohol 50 ml., prepared just before use and not filtered. Rinse in 70% alcohol and differentiate with an alcoholic extract of saffron (2 g. saffron pistils in 100 ml. 90% alcohol at 60°C. for 6 hr.) while observing the progress of differentiation microscopically. Dehydrate by dropping a 0.1 % solution of acetic acid in absolute alcohol on the section for 30 sec., followed by pure absolute alcohol, xylene, and covering in balsam.     

A Urea Silver Nitrate Method for Nerve Fibers and Nerve Endings

A silver nitrate stain for nerve fibers and endings applicable to paraffin sections on the slide utilizes the properties of urea to accelerate the procedure and improve the specificity of the stain. After removal of the paraffin the sections are run through absolute, 95% and 80% alcohol and placed for 60-90 minutes at 50-60°C. in: 1% aqueous silver nitrate, 100 ml.; urea, 20-30 g.; 1g. mercuric cyanide and 1 g. picric acid in 100 ml. of distilled water, 1-3 drops. After the silver bath they are rinsed quickly in 2 changes of distilled water and reduced for 3-5 minutes at 25-30°C. in: water, 100 ml.; sodium sulfite, anhydrous, 10g.; hydroquinone, 1-2g.; urea, 20-30g. They are then washed thoroughly in 4-5 changes of distilled water, passed through graded alcohols into 80% alcohol and examined under the microscope. If nerve fibers are not distinct, the sections are returned to the same urea-silver-nitrate bath for 10-15 minutes, rinsed, reduced, washed and dehydrated as before. This process may be repeated until staining is adequate; then they are dehydrated, cleared, and mounted.

Nerve fibers show a color range from brown to black; nerve cells from yellow to brown; and the background, depending on the type of tissue and its fixation, from yellow to light brown.     

Simultaneous determination of acetylsalicylic acid and salicylic acid in human plasma by high-performance liquid chromatography

A high-performance liquid chromatographic (HPLC) method is described for the simultaneous determination of acetylsalicylic acid (ASA) and its main metabolite salicylic acid (SA) in human plasma. Acidified plasma is deproteinized with acetonitrile which is separated from the aqueous layer by adding sodium chloride. ASA and SA are extracted into the acetonitrile layer with high yield, and determined by reversed-phase HPLC (column: Novapak C₁₈ 4 μm silica,150×4mm I.D.; eluent: 740 ml water, 900 μl 85% orthophosphoric acid, 180 ml acetonitrile) and photometric detection (237 nm). 2-Methylbenzoic acid is used as internal standard. The method allows the determination of ASA and SA in human plasma as low as 100 ng/ml with good precision (better than 10%). The assay was used to determine the pharmacokinetic parameters of ASA and SA following oral administration of 100–500 mg ASA in healthy volunteers.