Routine Mayer's Hematoxylin and Eosin Stain (H&E)
Manual of Histologic Staining Methods of the Armed
Forces Institute of Pathology (Third Edition). American Registry
of Pathology ( Luna, Lee G., HT(ASCP) (editor)), McGraw Hill Publishers,
New York 1960
(Progressive Stain)
- Summary
- Mayor's hematoxylin is used because it eliminates the necessity for
differentiation and bluing of the section. It can be considered a progressive
stain which produces a stained section with a clearly defined nuclei while
the background is completely colorless.
The biggest objection to Mayer's
hematoxylin as used in the past, has been that stained slides often fade
after 1 to 3 years. This problem can be eliminated, however, when the slides
are washed, after the hematoxylin, in running water for a minimum of 20
minutes.
This method gives consistent results even when more than one person
stains sections from the same block. Also, slides may be left in the hematoxylin
for hours with-out overstaining. Because of the simplicity of the technique,
it is possible to teach others to use it within a shorter time as well
as a definite reduction in time performance of the stain itself.
- Fixation
- Any well fixed tissue.
- Technique
- Paraffin, celloidin, or frozen
- Solutions
-
- Mayer's Hematoxylin
- Eosin Solutions
- Gram's or Lugol's Iodine
- Staining Procedure
-
- Deparaffinize and hydrate to water
- If sections are Zenker-fixed, remove the mercuric chloride crystals
with iodine and clear with sodium thiosulphate
(hypo)
- Mayer's hematoxylin for 15 minutes
- Wash in running tap water for 20 minutes
- Counterstain with eosin from 15 seconds to 2 minutes depending
on the age of the eosin, and the depth of the counterstain desired. For
even staining results dip slides several times before allowing them to
set in the eosin for the desired time
- Dehydrate in 95% and absolute alcohols, two changes of 2 minutes
each or until excess eosin is removed. Check under microscope
- Clear in xylene, two changes of 2 minutes each
- Mount in Permount or Histoclad
- Results
- Nuclei - blue - with some metachromasia
Cytoplasm - various shades of pink-identifying different tissue components
- Remarks
- The adhesives used to attach sections onto the slides (gelatin,
egg albumen) will sometimes stain, in areas around the section,
with Mayor's hematoxylin. This will give the slides a slightly dark appearance
but in no way affects the nuclear staining. To remedy this, use 10-12%
glacial acetic acid in 95% alcohol, to "clean" the slides after Mayor's
hematoxylin. Following with a few dips in saturated aqueous lithium carbonate,
the nuclei will blue immediately. This is optional, for the 20-minute wash
in running water is sufficient to blue the nuclei. This step will in no
way alter or minimize the staining of the nuclei.
- Reference
- Histopathology Laboratories, Armed Forces Institute
of Pathology, Washington, D.C. 20305.
Gomori's One-StepTrichrome Stain
Gomori,Sheehan and Hrapchak in: Histotechnology
A Self-Instructional Text; ASCP Press. American Society of Clinical
Pathologists Chicago 1990
- Purpose
- To identify an increase in collagenous connective tissue fibers, or to differentiate between collagen and smooth muscle fibers
-
- Principle
- In the one-step trichrome procedure, a plasma stain (chromotrope
2R) and a connective tissue fiber stain (fast green FCF, light green, or
aniline blue) are combined in a solution of phosphotungstic acid to which
glacial acetic acid has been added. Phosphotungstic acid favors the red
staining of muscle and cytoplasm. The tungstate ion is specifically taken
up by collagen, and the connective tissue fiber stain is subsequently bound
to this complex, coloring the collagen green or blue, depending on the
counterstain used.
- Fixative
- Any well-fixed tissue may be used. Bouin's solution is used
as a mordant to intensify the color reactions.
- Equipment
- 56 to 58 °C oven
- Coplin jars
- Erlenmeyer flasks
- graduated cylinders
- pipettes.
- Technique
- Cut paraffin sections at 4 to 5 mm.
- Quality Control
- Practically every tissue has an
internal control, so no other control sections are needed; however, if
a control is desired, uterus, small intestine, appendix, or fallopian
tube will provide good material.
- Reagents
-
- Bouin's Solution
- Picric acid, saturated aqueous solution .... 75.0 mL
- Formaldehyde, 37% to 40% ….. 25.0 mL
- Glacial acetic acid ….. 5.0 mL
- Weigert's Iron Hematoxylin
- Solution A
- Hematoxylin..... 10.0 g
- Alcohol, 95% ..... 1,000.0 mL
- Solution B
- Distilled water ..... 475.0 mL
- Hydrochloric acid, concentrated ..... 5.0 mL
- Ferric chloride, 29% solution ..... 20.0 mL
- Working Solution
- Mix equal parts of solutions A and B.
- Gomori's Trichrome Stain
- Chromotrope 2R (Baker No. 5-F703) . . . . . 0.6 g
- Fast green FCF, light green or aniline blue ..... 0.3
g
- Phosphotungstic acid ..... 0.8 g
- Glacial acetic acid . . . . . 1.0 mL
- Distilled water ..... 100.0 mL
- Store this solution in the refrigerator.
- 0.5% Acetic Acid Solution
- Glacial acetic acid ..... 0.5 mL
- Distilled water ..... 99.5 mL
- Procedure
-
-
- Deparaffinize sections and hydrate to distilled water.
- Rinse well in distilled water.
- Mordant sections in Bouin's solution for I hour at
56 °C.
- Remove slides from the oven, allow to cool, and wash
in running water until the yellow color disappears.
- Rinse in distilled water.
- Stain sections in Weigert's hematoxylin for 10 minutes.
- Wash in running water for 10 minutes.
- Stain sections for 15 to 20 minutes in Gomori's trichrome
stain.
- Differentiate for 2 minutes in 0.5% acetic acid.
- Dehydrate, clear, and mount with synthetic resin.
- Results
- Nuclei..... black
Cytoplasm, keratin, muscle fibers ..... red
Collagen and mucus ..... green or blue
- Remarks
- Sweat et al state that coloration of fine connective tissue fibers
is affected by the dye solution pH, with maximum binding occurring around
pH 1.3. The pH of Gomori's trichrome is about 2.5, which decreases affinity
for anions by approximately 50%, so these investigators suggest that by
replacing the acetic acid with hydrochloric acid, a pH of approximately
1.3 can be obtained. The intensity of coloration of the fine connective
tissue fibers can be varied by altering the pH.
Verhoeff's Elastic Stain
Mallory, Sheehan and Hrapchak in:Histotechnology - A
Self-Instructional Text ASCP Press. American Society of Clinical Pathologists,
Chicago 1990
- Purpose
- Elastic fiber techniques are used for
the demonstration of pathologic changes
in elastic fibers. These include atrophy of the elastic tissue, thinning
or loss that may result from arteriosclerotic
changes, and reduplication, breaks, or splitting that may result from other
vascular diseases. The techniques also may be used to demonstrate normal
elastic tissue, as in the identification of veins and arteries, and to
determine whether or not the blood vessels have been invaded by tumor.
- Principle
- The tissue is overstained with a soluble lake of
hematoxylin-ferric chloride-iodine. Both ferric chloride and iodine serve
as mordants, but they also have an oxidizing function that assists in converting
hematoxylin to hematein. The mechanism
of dye binding is probably by formation of hydrogen bonds, but the exact
chemical groups reacting with the hematoxylin have not been identified.
This method requires that the sections be overstained and then differentiated,
so it is regressive. Differentiation is accomplished by using excess mordant,
or ferric chloride, to break the tissue-mordant-dye complex. The dye will
be attracted to the larger amount of mordant in the differentiating solution
and will be removed from the tissue. The elastic tissue has the strongest
affinity for the iron-hematoxylin complex and will retain the dye longer
than the other tissue elements. This allows other elements to be decolorized
and the elastic fibers to remain stained. Sodium thiosulfate is used to
remove excess iodine. Van Gieson's solution is the most commonly used counterstain,
but others may be used.
- Fixative
- Any well-fixed tissue may be used.
- Equipment
-
- Mechanical stirrer
- Coplin jars
- Erlenmeyer flasks
- graduated cylinders.
- Technique
- Cut paraffin sections at 4 to 5 mm.
- Quality Control
- Use a section of aorta embedded
on edge, or a cross section of a large artery.
- Reagents
-
- Lugol's Iodine
..... 10.0 g
- Potassium iodide ..... 20.0 g
- Distilled water .....
1,000.0 mL
- Put the iodine and potassium iodide in a flask with 200
mL of the water. Stir on a mechanical stirrer until the iodine dissolves
and then add the remaining water.
- 100% Ferric Chloride
- Ferric chloride ..... 50.0 g
- Distilled water ..... 500.0 mL
- Store in the refrigerator.
- Verhoeff’s Elastic Stain
Prepare fresh each time and mix in order:
- Hematoxylin, 5% in 95% alcohol (may be kept as a stock
solution) ..... 30.0 mL
- Ferric chloride, 10% solution ..... 12.0 mL
- Lugol's iodine ..... 12.0 mL
- Van Gieson's Solution
- Acid fuchsin, 1% aqueous ..... 20.0 mL
- Picric acid, saturated solution (14 g/L) ..... 380.0 mL
- 5% Sodium Thiosulfate
(Sodium thiosulfate ..... 50.0 g + Distilled water .....
1,000.0 mL)
- Procedure
-
- Deparaffinize sections and hydrate to distilled water.
- Place sections in Verhoeff’s elastic tissue stain for
I hour.
- Wash in two changes of distilled water.
- Differentiate sections microscopically in 2% ferric chloride until the
elastic fibers are distinct and the background is colorless to light gray.
If the sections are differentiated too far, restain.
- Rinse sections in distilled water.
- Place sections in sodium thiosulfate for I minute.
- Wash in running tap water for 5 minutes.
- Counterstain sections in van Gieson's stain for 1 minute.
- Differentiate
in 95% alcohol.
- Dehydrate in absolute alcohol, clear in xylene,
and mount with synthetic resin.
- Results
- Elastic fibers..... blue-black to black
Nuclei ..... blue to black
Collagen..... red
Other tissue elements ..... yellow
- Notes
-
- It is easy to overdifferentiate this stain. If the background is completely colorless, so that a clear
yellow counterstain is obtained, the section may be overdifferentiated.
It is probably better to err on the side of underdifferentiation.
- Overdifferentiated sections may be restained at any
step provided they have not been treated with alcohol.
- Do not prolong staining with van Gieson's
solution as picric acid also will differentiate the stain further.
- It is not necessary to remove mercury deposits before
staining, as they will be removed by the staining solution.
- The preparation of van Gieson's solution is critical
for proper differentiation of muscle and collagen. If the picric acid is
not saturated, collagen will not stain red, and cytoplasm, muscle, and
collagen may all stain the same color.
- To prepare the Verhoeff’s elastic staining solution, the reagents must be added in the order given, with mixing after each addition, or poor staining may result.
- The staining
jar that contained the Verhoeff’s solution may be cleaned easily by transferring
the 2% ferric chloride to the jar for a few minutes before discarding the
solution.
- For optimum results, slides must be individually differentiated,
as the time of differentiation is somewhat dependent on the amount of elastic
tissue present. Do not depend on the control for timing the differentiation
of all sections.
PAS Reaction with Diastase Digestion
Manual of Histologic Staining Methods of the Armed Forces Institute of Pathology (Third Edition). American Registry of Pathology ( Luna, Lee G., HT(ASCP) (editor)), McGraw Hill Publishers, New York 1960
- Purpose
- The demonstration of glycogen in tissue sections.
- Principle
- This is a very sensitive histochemical method for glycogen.
Diastase and a-amylase act on glycogen to depolymerize it into smaller
sugar units (maltose and glucose) that are washed out of the section. The
Schiff reaction has been described in the PAS procedure.
- Fixative
- 10% neutral buffered formalin, formalin alcohol, or
absolute alcohol.
- Equipment
-
- Hot plate pH meter
- Coplin jars
- balance
- Erlenmeyer
flasks
- graduated cylinders
- filter paper
- Technique
- Gut two paraffin sections at 4 to 5mm.
Label one section "with" and one section "without."
- Quality Control
- Two control sections of liver containing glycogen
must be used, one labeled "with" and one labeled "without."
- Reagents
-
- 0.5% Periodic Acid
- Periodic acid ..... 2.5g
- Distilled water ..... 500.0 ml
- IN Hydrochloric Acid
- Hydrochloric acid, concentrated (specific gravity, 1.19) ..... 83.5
mL
- Distilled water ..... 916.5 mL
Add the acid to the water and mix well.
- Schiff Reagent
- Distilled water ..... 800.0 mL
- Basic fuchsin ..... 4.0 g
- Sodiumetabisulfite ..... 4.0 g
IN hydrochloric acid ..... 80.0 mL
Heat the water to the boiling point. Remove from flame, add the basic
fuchsin, and reheat to the boiling point. Cool the solution to 50 °C
and Filter. Add 80.0 mL of IN HCI,
cool completely, and add 4.0 g of sodium metabisulfite. Place the solution
in the dark overnight. The solution should be light amber after standing.
Add 2.0 g of activated charcoal and shake for I minute. Filter and store
the solution in the refrigerator.
- Test for Quality of Schiff Reagent
(See the PAS procedure in this chapter.)
- 0.55% Potassium Metabisulfite
- Potassium metabisulfite ..... 2.75 g
- Distilled water ..... 500.0 mL
- Malt Diastase Solution
- Diastase of malt ..... 0.1 g
- Phosphate buffer, pH 6.0 ..... 100.0 mL
- Phosphate buffer, pH 6.0
- Sodium chloride ..... 8.0 g
- Sodium phosphate, monobasic . .. .. 1.97 g
- Distilled water . .. .. 100.0 mL
- Adjust pH to 6.0 if necessary.
- Procedure
- Deparaffinize and hydrate slides to distilled water.
- Place the sections labeled "with" in preheated diastase solution
at 37 °C for I hour. Hold the sections labeled "without" in distilled
water.
- Wash in running water for 5 minutes.
- Place all sections ("with" and "without") in 0.5% periodic acid solution
for 5 minutes.
- Wash in three changes of distilled water.
- Place in Schiff reagent for 15 minutes.
- Wash for 1 minute in each of two jars of 0.55% potassium metabisulfite
to remove excess stain.
- Wash in running tap water for 10 minutes to develop full color.
- Counterstain ½ minute
in Harris's hematoxylin with acetic acid (2 mL acetic acid/48 mL hematoxylin).
- Wash well in running water to blue the hematoxylin.
- Dehydrate with two changes each of 95% and absolute
alcohol, clear with xylene, and mount with synthetic resin.
- Results
- Glycogen will stain bright rose red on the section labeled
"without" and will be absent from the section labeled "with."
- Notes
- Malt diastase, containing both a- and (3-amylase, is commonly
used for digestion but tends to loosen the sections. For this reason as
well as the decreased digestion time, many laboratories prefer to use human
saliva, which contains only a-amylase. If preferred, digest with saliva
for 20 minutes at room temperature.
- Glycogen fixed in picric acid-containing fixatives may be
more resistant to diastase digestion than when digestion follows other
fixatives (Sheehan and Hrapchak).
Routine Paraffin Cytoplasmic, Membrane Antigens and Nuclear Antigens
-
Purpose
- Immunohistochemistry
is used to identify a long list of antigens. It is a very effective and
flexible technique that is dependent upon the specificity and sensitivity
of the primary antibody. If one has an antibody that identifies the fixed,
processed antigen, any number of secondary antibodies and/or amplification
techniques can be used to identify the antigen in paraffin sections.
- Principle
- The tissue is processed and unstained paraffin sections
are mounted on glass slides. Most procedures call for "antigen retrieval"
using microwave ovens and citrate buffers. The incubation in methanol and
hydrogen peroxide is designed to "kill" the endogenous peroxidases and
eliminate background staining. The appropriate dilution of primary antibody
is placed in solution on the deparaffinized sections and exposed of an
appropriate time interval (depending on the affinity and avidity of the
antibody and the preservation and concentration of the antigen). The secondary
antibody systems are then placed on the slide. The procedures provided
below illustrate the use of the ABC kits but many different protocols,
signal amplification systems and indicator systems are available. The new
mouse-on-mouse systems permit the use of some mouse monoclonal antibodies
on mouse tissue.
- Fixative
- In general, tissue fixed in paraformaldehyde for less than
48 hours provides the best results. However, different antigens will require
different protocols. Post fixation of fomalin or paraformaldehyde fixed
tissue with B5 or other heavy metal fixative can "retrieve" some antigens.
The protocol for Mouse-on-Mouse used on the slide set is found by
clicking here.
Paraffin mounted slides
- Xylene 5 min.
- Xylene 5 min.
- Xylene/Lugol’s 4 min. *
- Absolute ETOH 3 min.
- Absolute ETOH 3 min.
- MEOH/H2O2(0.3%) 20 min.
- Absolute ETOH 1 min.
- 95% ETOH 2 min.
- 70% ETOH 2 min.
- H2O (running) 2 min.
- Dist. H2O 2 min.
- PBS (x2) 5 min.
- Normal Equine Serum 10% 20 min.<
- Primary abs. (Dilutions vary) Overnight
- PBS (x2) 5 min.
- Equine Anti-Mouse Biotin Conjugate 60 min.
- PBS (x2) 5 min.
- ABC - Elite 30 min.
- PBS (x2) 5 min.
- DAB (Vector-Brown) 3-5 min.
- Mayer’s Hematoxylin 1 min.
- Tap H2O 5-10 min.
- Dehydrate, clear and coverslip
- *B5 Fixed Tissue only
- NOTE: Tissue sections are placed in a 55 Celsius oven for
30 minutes or overnight.
Immunoperoxidase Staining (Nuclear Antigens)
- Xylene 5 min. RoomTemp.
- Xylene 5 min. RoomTemp.
- ETOH 3 min. RoomTemp.
- ETOH 3 min. RoomTemp.
- H202 + 3% Methanol 20 min. RoomTemp..
- ETOH 2 min. RoomTemp.
- ETOH 2 min. RoomTemp..
- H2O tap 5 min. RoomTemp..
- distilled H2O 5 min. RoomTemp..
- Citrate Buffer 4 min. microwave*
- Citrate Buffer 4 min. microwave*
- Citrate Buffer 4 min. microwave
- Cool down 15 min. RoomTemp
- PBS 5 min. RoomTemp
- PBS 5 min. RoomTemp.
- N horse serum 20 min. RoomTemp.
- Primary antibody overnight 4 C
- PBS 5 min. RoomTemp.
- PBS 5 min. RoomTemp.
- Secondary (BHAM) 1:800 60 min. RoomTemp.
- PBS 5 min. RoomTemp.
- PBS 5 min. RoomTemp.
- Tertiary ABC 1:50 30 min. RoomTemp.
- PBS 5 min. RoomTemp.
- PBS 5 min. RoomTemp.
- DAB 3-5 min. RoomTemp.
- H2O running tap 5 min. RoomTemp.
- Hematoxylin-Mayers 30 seconds RoomTemp.
- H2O running tap
- Dehydrate, clear, coverslip