Freezing by Liquid Carbon Dioxide in Making Slides Permanent

The expansion of liquid CO₂ may be employed in a quick-freeze method for making aqueous slide preparations permanent. An apparatus is described for this purpose which could be duplicated satisfactorily by cutting a 22mm square hole in the top of a standard freezing microtome specimen holder. The edges should be filed smooth to provide a flat surface for the slide to rest on, and clamps added to keep the slide in place while freezing. Once the slide is frozen, the cover slip may be readily removed, leaving practically all of the tissue on the slide. Following simultaneous thawing and dehydration of the slide in 95% alcohol, covering is done with Diaphane or Euparal and a clean, dry cover slip.     

An Abrasive Paper Technique for Preparing Sections of Wood for Microscopic Study

Dry wood specimens are sawed to 2mm thickness and impregnated with resin such as Lewisol 28 (Hercules Powder Co.). One side of the specimen is ground by hand on abrasive papers of grades #100, #180, #240, and #320. This side is then cemented to a petrographic glass slide with stick shellac and the other side similarly ground. Scratches can be eliminated by scraping the ground surface with the sharp edge of an ordinary glass microscopic slide. The section is removed by heating the slide, dissolving the shellac with alcohol and the resin of the embedding matrix with xylene. The sections can be stained in a hot saturated alcoholic solution of safranin O, counterstained with 0.01% fast green in an equal parts mixture of clove oil, methyl cellosolve, and absolute alcohol, and mounted in balsam.     

Producing Frozen Sections of Calcified Bone

We describe a procedure for the rapid production and maintenance of fresh frozen bone biopsies which can be used for a variety of immunohistochemical techniques. Within 5 min of excision. tissue is placed in cold 5% polyvinyl alcohol, surrounded with 3% carboxymethylcel-lulose in a hand made aluminum foil embedding mold and frozen by immersion in an absolute ethanol/dry ice slurry at -70 C. The tissue block is attached to the specimen stub with cryocom-pound and installed in a -32 C cryostat whose tungsten carbide D profile knife is maintained at -70 C. Automatic controls are set at a slow cutting speed and the “sectioning window” is adjusted to fit the biopsy size. Knife angle, thickness gauge and antiroll bar are changed to produce a complete section. The block face is smoothly “papered” with a polyvinylpyrrolidone (PVP) impregnated Ross lens paper strip. A single section is cut and positioned on a sequentially numbered, acid cleaned, double dipped chrome-alum gelatin coated slide: adhesion is aided by “press-blotting” with bibulous paper. Sections are stored at -20 C or in a desiccator at room temperature. A brief fixation followed by removal of the water soluble PVP and lens paper generates fresh frozen bone sections suitable for further analysis.     

Concentrating and Staining Bone Marrow; An On-the-Slide Technique

A 0.5-1 ml sample of bone marrow is aspirated into a syringe containing 3 drops of 15% K₂-EDTA and an additional 1-2 drops of the EDTA solution previously placed on a slide, is then drawn into the syringe. All of the contents are ejected onto this slide, which is carefully tilted 2 or 3 times to an angle of 5-10°, and the edge brought to the center of another slide. The slide with the aspirate is then slowly tilted to 80-90°. Most of the blood and part of the marrow will drain off, leaving spicules of marrow and some blood on the original slide. A small drop of this concentrated marrow is dragged off with the edge of a third slide and deposited about 2 cm from the edge of a fourth slide on which the smear is to be made. The smear is made by bringing a clean (smearing) slide to the slide with the deposited marrow with flat surfaces parallel and the edges at a 90° angle. With gentle pressure, the smearing slide is pushed toward the empty end of the slide upon which the smear is made. This separates the marrow from the circulating blood. Before staining the smear is air dried and heated in an oven at 120-125 C for 2 min; or alternately for satisfactory but less uniform results the smear is heated over a microburner for 10 sec; then the smear is covered with 1 part of undiluted Wright's stain for 30—45 sec which is then diluted with 2 parts of a solution of 0.1-0.2 gm of Na₂S₂O₃ in 1 liter of distilled water and stained for 10-13 min with this diluted stain. Smears made in this manner have 3 concentric zones; the central zone contains the myeloid tissue; the middle, erythropoetic tissue; the outer, a mixture of blood and marrow.     

Restoration of broken cytology slides and creation of multiple slides from a single smear preparation.

A technique was developed for restoring broken cytology slides so that they are close to their original condition and for making multiple slides from a single smear preparation. The method is applicable to both cytologic preparations and histologic sections. In this study the fragmented smear preparation was treated with Pro-Texx, which penetrated, impregnated and solidified the full thickness of the pieces of the smear, enabling them to be lifted from the pieces of the broken slide. The removed pieces of the smear preparation were reassembled onto a new slide, which was then restained and coverslipped. In preparing multiple teaching slides, the treated smear preparation was divided as planned, with each portion mounted onto a separate slide, which was then restained and coverslipped. Ten other fine needle aspiration cases with broken slides have been restored, and more teaching slides were prepared from a single smear preparation using the same technique. All were equally successful. This technique provides an excellent method of smear transfer in cases of broken slides and creation of multiple slides from a single smear preparation for cytology teaching. This is particularly useful for unusual cases.     

Using Scrapings from Formalin-Fixed Tissues to Diagnose Leptospirosis by Fluorescent-Antibody Techniques

Small specimens of formalin-fixed tissues approximatey 1 × 1 × 0.2 cm were cut from the suspect specimen. Several clean microscope slides were dipped in 1% aqueous gelatin and air-dried or dried on a slide warmer. Each tissue specimen was washed in running tap water for 2-5 min and then lightly scraped with a straight knife blade, cutting edge perpendicular to the surface of the specimen. The scrapings were allowed to build up and cling to the knife blade, which was then turned so that the broad surface contacted the slide; thus, the scrapings could be smeared onto the slide in a single motion. Sufficient pressure was applied to embed the tissue fragments in the gelatin coating. Smears, dried in air or on a slide warmer, were stained immediately by a standard direct or indirect technique to detect fluorescein-labeled antigens. This scraping method, adapted to the study of leptospirosis by fluorescent-antibody technique, could reduce the need for cryostat-cut tissues and facilitate the observation of individual leptospires.     

A standardized method for identifying and counting the vagile and sessile periphyton

Summary A technique adapting the traditional slide method for quantitative study of periphyton populations is described. A substrate of known area and composition (a microscope slide) is exposed to colonization by periphyton in a body of water. At the end of the exposure time the periphyton is fixed while still on the slide and (as suggested by Bodian) impregnated with protargol. This impregnation reveals clearly all the autotrophic and heterotrophic forms in the periphyton population. The entire population is thus permanently preserved for study.Dedicated to Prof. Rolf Danneel on the occasion of his 75th birthday     

Three-dimensional scaffold containing EGF incorporated biodegradable polymeric nanoparticles for stem cell based tissue engineering applications

Stem cell-based tissue engineering holds much hope for the development of multifunctional tissues to replace diseased organs. The attachment and survival of stem cells on a three-dimensional (3D) scaffold must be enhanced for faster progression of stem cell based tissue engineering. This study evaluate the stability of mesenchymal stem cells (MSCs) in 3D porous scaffolds composed of a collagen and chitosan blend impregnated with epidermal growth factor incorporated chitosan nanoparticles (EGF-CNP). The EGF-CNP scaffolds were characterized by transmission electron microscopy, which revealed that the nanoparticles were round in shape and 20 ∼ 50 nm in size. The scaffolds were prepared by freeze drying. A Fourier-transform infrared spectrum study revealed that the linkage between collagen and chitosan was through an ionic interaction. Thermal analysis and degradation studies showed that the scaffold could be used in tissue engineering application. MSCs proliferated well in the EGF-CNP impregnated scaffold. A scanning electron microscope study showed anchored and elongated MSCs on the EGF-CNP impregnated scaffold. A 3D biodegradable collagen chitosan scaffold impregnated with EGF-CNP is a promising transportable candidate for MSC-based tissue engineering, and this scaffold could be used as an in vitro model for subsequent clinical applications.     

A Numbered-Grid Locator Slide for Relocating Microscopic Fields

Four strips of drawing paper, each 22 × 30 cm, are taken. Numbers are typed from a typewriter with elite type face in such a way that, when pasted side by side along their lengths on another sheet of drawing paper, they yield a 88 × 30 cm master copy carrying numbers commencing from 1001 at top left and ending with 6680 at bottom right, each number preceded and succeeded by a dot. The upper and lower edges of this rectangle containing these figures are then extended by lines 2 cm each to the left and the ends jointed to make up a 90 × 30 cm master copy from which a 3 × 1 inch (7.5 × 2.5 cm) slide is prepared by photographic reduction. To use this slide, the microscopic field is found, the slide carrying the tissue is exactly replaced by the locator slide, and the number recorded. For subsequent reference, the procedure is reversed by first finding the number and then replacing the locator slide by the one bearing the tissue     

Scanning electron microscopy of mitotic nuclei and chromosomes in filamentous fungi

A new method for scanning electron microscopy (SEM) of fungal mitotic nuclei and chromosomes was established for two ascomycetes, Cochliobolus heterostrophus and Neurospora crassa. Nuclei and chromosomes discharged from germling cells by the germ-tube burst method were spread on a surface of a glass slide. The spreads were impregnated with osmium-thiocarbohydrazide for conductive staining, followed by coating with platinum, and observed by field-emission SEM. Ultrastructure of fungal chromosomes and nuclei was visualized by SEM for the first time.     

Laser Capture Microdissection - A Demonstration of the Isolation of Individual Dopamine Neurons and the Entire Ventral Tegmental Area

Laser capture microdissection (LCM) is used to isolate a concentrated population of individual cells or precise anatomical regions of tissue from tissue sections on a microscope slide. When combined with immunohistochemistry, LCM can be used to isolate individual cells types based on a specific protein marker. Here, the LCM technique is described for collecting a specific population of dopamine neurons directly labeled with tyrosine hydroxylase immunohistochemistry and for isolation of the dopamine neuron containing region of the ventral tegmental area using indirect tyrosine hydroxylase immunohistochemistry on a section adjacent to those used for LCM. An infrared (IR) capture laser is used to both dissect individual neurons as well as the ventral tegmental area off glass slides and onto an LCM cap for analysis. Complete dehydration of the tissue with 100% ethanol and xylene is critical. The combination of the IR capture laser and the ultraviolet (UV) cutting laser is used to isolate individual dopamine neurons or the ventral tegmental area when using PEN membrane slides. A PEN membrane slide has significant advantages over a glass slide as it offers better consistency in capturing and collecting cells, is faster collecting large pieces of tissue, is less reliant on dehydration and results in complete removal of the tissue from the slide. Although removal of large areas of tissue from a glass slide is feasible, it is considerably more time consuming and frequently leaves some residual tissue behind. Data shown here demonstrate that RNA of sufficient quantity and quality can be obtained using these procedures for quantitative PCR measurements. Although RNA and DNA are the most commonly isolated molecules from tissue and cells collected with LCM, isolation and measurement of microRNA, protein and epigenetic changes in DNA can also benefit from the enhanced anatomical and cellular resolution obtained using LCM.     

A Method for Applying Different Stains to Alternate Serial Sections On a Single Microscope Slide

Every other section on the slide is coated with an inert grease (Dow Corning 7 Compound). The first staining technique is applied, thus staining the sections not covered with grease. The grease is dissolved in xylene, the slide rehydrated, and the sections already stained are coated with grease. The second staining technique is applied, and the grease is again dissolved in xylene, yielding finally a slide on which alternate sections have been stained by the two different staining techniques. Silicone greases, applied with a syringe and blunt hypodermic needle, are useful coating materials because of their insolubility in water and alcohol, chemical inertness, and heat stability. Silicone coatings are compatible with most staining techniques, including those which use strong oxidants, reductants, acids, bases, enzymes, and high temperatures. The method is particularly useful in examining serial sections of small blocks of tissue, or of tissues varying significantly in structure every few sections.     

A novel technology allowing immunohistochemical staining of a tissue section with 50 different antibodies in a single experiment.

Immunohistochemical (IHC) examination is frequently necessary for a histological differential diagnosis of tumors. To simplify IHC examination, we have developed a novel device called a "multiplex-immunostain chip (MI chip)." The chip is a panel of antibodies contained in a silicon rubber plate that consists of 50 2-mm-diameter wells. A tissue section slide is placed on the plate and is fastened tightly with a specially designed clamp. The plate with the slide is then turned upside down, which applies the antibodies to the section. This technology allows IHC staining of a tissue section with 50 different antibodies in a single experiment, reducing the time, effort, and expense of IHC analysis. In addition, it enables pathologists to compare expression of multiple antigens on a tissue section simply by changing microscopic fields on a single slide. These features are unique to the MI chip technology. The method requires no expensive instruments. This device can be used in various applications in differential diagnosis of tumors and the field of cell biology.     

Ultrastructural analysis of preparations impregnated with silver salts]

The work was devoted to the ultrastructural analysis of the neurohistological preparations. Sections of the tissue from the precardial parts of the pulmonary and caval dog veins were impregnated with silver salts after Campos and embedded in the araldite by a special method. Electronmicroscopi studies showed reduced silver adsorbed by the tissue of the impregnated preparations to exhibit a granular structure (the granules were 30-400 A in size). The largest of them were revealed in the axoplasm of the myelinated and unmyelinated nerve conductors, whereas the smaller ones found in various cellular and fibrous formations of the tissue substrate; silver granules were as a rule absent within the thickness of the myelin sheath. The noted regularities of adsorption and distribution of the silver granules in the impregnated preparations caused a morphologically expressed phenomenon of argentophilia.     

Improved Methods for Permanent Chromosome Preparations: Cellophane Squashes and Citric Acid Dissociation

Normally, squash preparations from prestained acetic acid softened or HCl macerated tissues are made by pressing the tissue under a coverglass (e.g. Walker 1973). When permanent slides are wanted the coverglass has to be removed sooner or later, which is only possible by hardening the squashed tissue by freezing, for example in carbon dioxide snow, or by slow diffusion of fixatives into the space between the slide and the coverglass. These methods are either expensive or time-consuming, and upon removal of the coverglass, many cells and chromosomes either are lost or are poorly preserved.     

Golgi impregnation with mercuric chloride: studies on the precipitate by X-ray powder diffraction and selected area electron diffraction

Summary An investigation was carried out to determine the nature of the precipitate in a technique which was originally proposed by Golgi and, later, modified by Cox, to stain nerve cells by the treatment of tissue with potassium dichromate and mercuric chloride.The approach was a twofold one: the study of the patterns of X-ray diffraction of successfully impregnated tissue and the analysis of electron diffraction patterns of selected areas of tissue where impregnated structures were observed.Evidence has been obtained that the precipitate, prior to the final alkalinization process, is mercurous chloride (calomel, Hg₂Cl₂). There appears to be no formation, at any time, of mercurous or mercuric chromate. The mercurous chloride is topographically associated exclusively with the presence of stained structures and cannot be detected in the non-stained background.Following the alkalinizing process necessary for the final darkening of the stained structures, the X-ray diffraction pattern of mercurous chloride usually was no longer detectable. It appears reasonable to assume that, when no crystalline compounds can be detected, metallic liquid mercury is formed.This study was supported by U.S. P.H.S. Grant NS 07998 and by the Medical Research Council of Canada. We are indebted to Mrs. K. Sörensen and Mr. A. Meier for technical assistance.     

Efficacy of mosquito nets treated with permethrin in Suriname

In the rain-forest of Suriname, where malaria is endemic, 95% of the Maroons (who call themselves bush-negroes) and all Amerindians use mosquito nets made of cotton cloth or, less frequently, nylon or cotton gauze over their hammocks or beds. Bush-negroes usually wash their nets weekly; Amerindians wash nets at 1-4 month intervals. Females of the principal local malaria vector, Anopheles darlingi Root, were seen blood-feeding through cotton cloth netting (at 22.30-23.30 hours) on a person sleeping in a hammock; others fed successfully after the net was opened in the morning. Cotton cloth impregnated with permethrin at a rate of 0.5 g/m2 killed all An. darlingi females exposed for 2 min, but after the material had been washed twice in soapy water the bioassay mortality fell to only 21.4%. Exit traps on a hut with a single sleeper protected by a permethrin-impregnated net yielded 185 An. darlingi females (12% blood-fed) in 74 nights, compared with 276 females (19% blood-fed) from another hut with a sleeper using an untreated net on the same nights (P less than 0.001). No An. darlingi females remained resting alive indoors in these huts during the daytime, and very few were found dead on the floor in the mornings (one treated, seven untreated). The 24 h mortality rate for those collected in exit traps was 58.4% for the test hut and 27.1% for the control hut (P less than 0.001). Bioassays of permethrin-treated cotton cloth using laboratory-reared sugar-fed Culex quinquefasciatus Say females showed that sprayed nets were less effective than nets impregnated by soaking (at equivalent dosages of 0.16-1.34 g/m2 measured by chemical assay) and confirmed that washing causes severe decline in insecticidal activity. The feasibility of local mass treatment of mosquito nets is discussed.     

Oriented Embedding of Biological Materials and Accurate Localization for Ultrathin Sectioning

Gelatin capsules with rounded ends clipped off and open ends moistened, affixed to a glass slide and sealed with a 15% gelatin solution are used to embed blocks of tissue in plastic. The surface of the slide serves as an orientation plane for structures of the tissue. The plane end of capsules of polymerized plastic containing no tissue is used in embedding frozen tissue sections. The plastic-infiltrated section is flattened against the capsule end under the weight of a 3/4 inch square of plate glass so that larger sections may be cut and surveyed. Embedding cultured cell monolayers grown on coverslips is accomplished in a comparable manner, but the square of plate glass is not needed as a weight. Block-face localization methods depend on the type of material embedded. With blocks of tissue it is achieved by moistening the face with xylene to develop relief. Thin tissue sections are examined by transmitted light, while cell monolayers are stained on the capsule end with methylene blue.     

Open-Face, Epoxy Embedding of Single Cells for Ultrathin Sections

Intact stamens of Tradescantia were fixed, dehydrated, and infiltrated with an epoxy resin. Each stamen was then put into a drop of resin on a microscope slide, which was transferred to the stage of a dissecting microscope so that individual hairs could be detached from the filament with fine tungsten needles. The detached hairs were transferred to drops of resin ca. 2 mm in diameter (6 or 7 in each of two rows) lying on a slide heavily coated with evaporated carbon. Polymerization was carried out in an oven until the resin attained a degree of viscosity that permitted orientation of the isolated hairs (by using a compound microscope) without their subsequent dislocation. When the small drops of resin had hardened after further polymerization, the positions of the hairs were marked by circumscribing the cells with India ink. The block was pried from the slide after rapid cooling with solid CO₂, and was then trimmed and sectioned. Cells suspended in culture medium were embedded in much the same way; they were centrifuged to obtain a pellet, which was fixed, dehydrated, and infiltrated. A small fragment of the pellet with a little resin was placed on a microscope slide, where the cells were dissociated under a dissecting microscope at ca. 100 × magnification. Individual cells were then picked up with tungsten needles and transferred to droplets of resin on a carbon-coated slide. The subsequent steps were similar to those described for the staminate hairs. Pieces of tissue in the 50-500 μ range were also handled by the foregoing technique. However, after infiltration they were put into large drops of resin on a slide coated with silicone mold-release rather than on a surface coated with carbon.     

High throughput slanted scanning whole slide imaging system for digital pathology

In whole slide imaging (WSI), normally only a one layer imaging of the slide is performed. Autofocus at multiple positions is usually required. But defocus blur still exists due to tissue folding or specimen thickness. Repeated Z-stack scan be applied here, which, however, is too time consuming. Here, a high throughput slanted scanning WSI system is reported. In this system, the slide surface was slanted 1° relative to the focal plane. Thus, the focal plane spanned multiple layers of the sample. By moving the slide, multi-layer image data of the sample can be acquired simultaneously at a time frame comparable to conventional 1-layer imaging. With image fusion, defocus blur can be avoided. High quality and fast imaging of both cytological and histological slide specimens was demonstrated without applying aberration correction. The system can be a highly efficient way for the application of WSI in digital pathology.