Hematology

 

CE: Phlebotomy    (May 1997)

We are receiving an increased number of under filled EDTA tubes, which causes continuing hematology problems in the lab.  Quality of results begins with sample collection. The small purple- topped tubes hold 2 ml. blood.   Two primary problems occur with under filled tubes:

           

            1.) The EDTA anticoagulant used is a liquid,

            which will dilute the results of the CBC.

           

            2.) Discrepancies in PCV results between the hematocrit centrifuge, and the Advia 120 and the Coulter T660 instruments  will occur.  The excess EDTA causes the RBCs to shrink, and they become crenated or have folded membranes.  Therefore the spun PCV is falsely lowered, while the diluent in the Advia and Coulter instruments causes the RBCs to swell to the correct size, giving a more accurate result.  

 

The recommendation is to fill the EDTA tubes at least halfway with blood, or use micro-collection tubes available in clin path.

 

 

CE Hematology    (October 1997)

Definition of Indices: The MCV index, MCHC index, and RDW index make up the indices of a CBC.

MCV: Mean cell (or corpuscular) volume, measured in cubic micrometers.  This is a directly measured parameter on the Advia 120 and T660 Instruments.  It is manually calculated by dividing the packed cell volume by the red cell count and multiplying by 10.  High MCV will occur in reticulocytosis, congenital macrocytosis of poodles, FeLV infected cats, and erroneously with agglutination.  Low MCV will occur in iron deficiency, portosystemic venous shunts, and the Akita breed.

MCHC:  Mean cell hemoglobin concentration, measured in grams per deciliter.  This is calculated by dividing the total hemoglobin by the hematocrit.  Also calculated automatically by the Advia 120.  Low MCHC will occur in reticulocytosis (immature hemoglobin), and iron deficiency.  High MCHC is almost always a result of in vivo and in vitro hemolysis, or laboratory error (a true increase in MCHC does not normally occur).

RDW:  Red cell distribution width, which is determined by the Advia 120 instrument.  It is the coefficient of variation of the red cell volume distribution.  It is an index of the degree of anisocytosis or variation in size of erythrocytes.  Anemias with significant microcytosis or macrocytosis will have increased RDW.  Reticulocytosis results in increased RDW.

 

Reference:

Duncan, Prasse, and Mahaffey, Veterinary Laboratory Medicine, 1994

 

 

Hematology by the Advia 120:   (February 2000)

The hemoglobin result is read photometrically.  This result, and the corresponding MCHC can be skewed because of lipemia in the blood.  Therefore, in lipemic and hemolyzed specimens, the more accurate Calculated Hemoglobin and CHCM are reported.  The Advia 120 determines the density and size of the red cells.  These parameters are not affected by lipemia.  The CHCM is derived from the Calculated Hemoglobin.  These parameters are reported in the “Tech comment” field.

 

 

 

CE Hematology:    (December 2001)

We have noticed unusual changes of RBC parameters in some of our “send-in” EDTA specimens for hematology in cats and dogs. A small study revealed that if the EDTA tubes stay at room temperature for 48 hours, an artificially induced macrocytosis might occur.  This was demonstrated on two hematology analyzers, the Advia 120 and the Coulter Counter S+lV  (no longer in use).  You may get false macrocytosis in normal cats and dogs, and possibly get false normocytosis in cats and dogs with microcytosis.  Since macrocytosis will increase the PCV, manually obtained PCVs will also be falsely elevated.

As a result, we recommend that cat and dog specimens should be run within 8 hours, or else

stored in the refrigerator until analyzed.  

 

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Refractometers (use and care):    (June  2002)     These should be checked daily with distilled or deionized water for a reading of 1.000.  Tap water is not appropriate.  Calibrate if the reading differs from 1.000 by more than ˝ of a division.

To insure a sharp line for reading results and to avoid scratching the prism, close the sample cover.

Fill the prism area by capillary action, making sure the prism is clean prior to filling, and avoid samples with lipemia or hemolysis.