Donor-specific B-cell tolerance after ABO-incompatible infant heart transplantation
Isotype-specific detection of ABO blood group antibodies using a novel flow cytometric method
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Transcript of Isotype-specific detection of ABO blood group antibodies using a novel flow cytometric method
Isotype-specific detection of ABO blood group antibodies usinga novel flow cytometric method
Naturally occurring antibodies (Ab) such as anti-A/B Ab play
an important role in transfusion and transplantation medicine.
The analysis of ABO antigens (Ag) and anti-A/B Ab prior to
blood product transfusion and organ transplantation is part of
the daily routine in blood bank laboratories. Ignoring the
ABO-blood group match between donor and recipient may
lead to life-threatening complications, such as haemolytic
transfusion reactions and (hyper) acute vascular graft rejec-
tion. ABO-specific Ab belong to the group of naturally
occurring Ab first described by Landsteiner (1901) and later
studied extensively by other groups (Avrameas, 1991; Cou-
tinho et al, 1995). Anti-A/B Ab formation requires the
presence of accessible Ag, which is provided by microorga-
nisms in the gastrointestinal tract (Springer & Horton, 1969).
Although ABO Ag have only subtle chemical differences, anti-
A/B are, in general, highly specific for their respective blood
group Ag (Rydberg, 2001; Watkins, 2001). Nevertheless,
despite this high specificity shown for anti A/B natural Ab, a
variety of mainly IgM Ab, including monoclonal anti-D, show
polyspecificity and polyreactivity to unrelated exo- and
autoantigens (Thompson et al, 1992; Thorpe & Bailey, 1993).
Anti-A/B Ab differ from most naturally occurring Ab in so far
as they are expressed exclusively in individuals lacking the
corresponding Ag. Hence, they are not auto-reactive. However,
human plasma contains naturally occurring autoantibodies to
several red blood cell (RBC) proteins including the anion
transport protein, band 3 (Lutz, 2004). ABO typing on whole
RBC populations with anti-human IgG does not interfere with
binding of anti-band 3 autoantibodies in situ, because anti-
band 3 autoantibodies bind to oxidatively stressed and
senescent RBC (Lutz et al, 1988).
Blood group typing depends on the detection of ABO Ag on
the surface of RBC by means of haemagglutinating antibodies
against the A or B Ag (Brecher, 2002). The quantification of
anti-A/B Ab is carried out most frequently by haemagglutina-
tion and haemolysis techniques. These techniques are based on
G. Stussi,1 K. Huggel,1 H. U. Lutz,2 U.
Schanz,3 R. Rieben4 and J. D. Seebach1
1Laboratory for Transplantation Immunology,
Department of Internal Medicine, University
Hospital Zurich, Zurich, 2Institute of
Biochemistry, ETH Hoenggerberg, Zurich,3Division of Haematology, Department of Internal
Medicine, University Hospital Zurich,
Switzerland, and 4Department of Clinical
Research, University of Bern, Bern, Switzerland
Received 10 March 2005; accepted for
publication 22 June 2005
Correspondence: PD Dr med. Jorg D. Seebach,
University Hospital Zurich, Department of
Internal Medicine, Laboratory for
Transplantation Immunology, Ramistrasse 100,
C HOER 31, CH-8091 Zurich, Switzerland.
E-mail: [email protected]
Summary
Several methods to detect anti-A/B antibodies based on haemagglutination
and haemolysis have been described. These methods measure predominantly
anti-A/B immunoglobulin (Ig)M, whereas anti-A/B IgG and IgG subclasses
are less well examined. We established a flow cytometry method (ABO-
fluorescence-activated cell sorting; ABO-FACS) to quantify binding of anti-
A/B IgM, IgG and IgG subclasses to human A or B red blood cells. Anti-A/B
IgM were present in the majority of 120 blood donors, as expected from
blood group typing. The sensitivity and specificity of anti-A/B IgM to predict
the blood group was 93% and 96% respectively. Anti-A/B IgG was found in
34/38 blood group O samples (89%). Anti-B IgG in blood group A or anti-A
IgG in blood group B was present in 4/28 (14%) and 1/28 (4%) samples,
respectively, and absent in 26 AB sera. IgG2 was the predominant IgG
subclass. The correlation of anti-A/B IgM and IgG in the ABO-FACS with
haemagglutination titres was 0Æ870 and 0Æ783, respectively (n ¼ 240;
P < 0Æ001) whereas the comparison of ABO-FACS with ABO-enzyme-
linked immunosorbent assay was less significant. In conclusion, ABO-FACS
is a valid method to quantify anti-A/B IgM, IgG and IgG subclasses. It opens
the possibility of isotype-specific monitoring of anti-A/B antibodies levels
after ABO-incompatible solid organ and stem cell transplantation.
Keywords: ABO blood group, antibodies, flow cytometry, enzyme-linked
immunosorbent assay, immunoglobulin G subclasses.
research paper
doi:10.1111/j.1365-2141.2005.05705.x ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963
crosslinking of standardised RBC by haemagglutinins in the
serum of interest. Yet, haemagglutinating Ab are predomin-
antly of the IgM class and the determination of anti-A/B IgG in
clinical practice is more challenging. A variety of assays have
been used for this purpose, making it difficult to compare the
results of different studies (Hershko et al, 1980; Sniecinski
et al, 1988; Bar et al, 1995; Nussbaumer et al, 1995). More-
over, none of these techniques allows the determination of IgG
subclasses. Therefore, several years ago an enzyme-linked
immunosorbent assay (ELISA)-based method, to measure the
binding of anti-A/B Ab to synthetic or animal-derived A and B
substances, was developed, enabling the discrimination
between IgM, IgG and IgG subclasses (Buchs & Nydegger,
1989; Rieben et al, 1991). However, this assay depends on the
binding to synthetic or animal-derived Ag, rather than the
actual human ABO Ag on RBC. We therefore developed a new,
semi-quantitative assay based on flow cytometry to determine
the binding of IgM, IgG and IgG subclasses to ABO Ag
expressed on RBC (ABO-fluorescence-activated cell sorting,
ABO-FACS). Using this method we measured the total amount
of anti-A/B Ab in 120 healthy blood donors and compared the
results with haemagglutination and the ABO-ELISA.
Materials and methods
Sera and red blood cells
The amount of anti-A/B Ab in the sera of healthy donors was
evaluated by measuring binding to human RBC. For this
purpose, 120 sera were obtained from the local transfusion
service and stored at )20�C (28 A, 28 B, 38 O, and 26 AB).
Blood group typing was performed by standard techniques and
all samples were negative for human immunodeficiency virus,
hepatitis B virus and hepatitis C virus. The mean age of the
blood donors was 50 years, ranging from 21 to 70 years. Forty-
six per cent were male and 76% were rhesus positive. Eighty-
eight per cent of blood group A or AB donors had the A1 or
A1B subgroup and the remainder had the A2 or A2B subgroup.
Statistical analyses of age, rhesus blood group and gender did
not reveal significant differences among the ABO blood groups
(data not shown). Rhesus negative human RBC of type A1, B,
and O were obtained from the local transfusion service.
Porcine RBC and serum were used as controls and were kindly
provided by the local slaughterhouse. The RBC were isolated
from heparinised venous blood and washed three times in
phosphate-buffered saline (PBS). To prevent haemagglutina-
tion, the cells were fixed according to a previously described
method (Pins et al, 1997). Briefly, 100 ll of highly concentra-
ted RBC (haematocrit 80%) were incubated for 20 min at 4�Cin 4 ml Karnovsky buffer, which contains formaldehyde and
glutaraldehyde. Thereafter, the RBC were washed once in PBS
containing 6% bovine serum albumin (BSA; Fluka Biochem-
icals, Buchs, Switzerland) and twice in PBS containing 0Æ6%BSA. After fixation a 1% solution of RBC was prepared
resulting in a concentration of 1–5 · 108 RBC/ml. RBC were
stored at 4�C and used for up to 6 weeks without changes in
Ab binding levels.
For antibody absorption, serum was incubated with washed,
non-fixed A, B, or O RBC at different ratios (106–108/ml) for
30 min at RT under rotation using a disc rotator (Fischer
Bioblock Scientific, Illkirch, France: 33 rpm). Subsequently the
samples were centrifuged for 4 min at 1700 g and the
supernatant was harvested. This procedure was performed
consecutively three times and the absorbed sera were tested by
ABO-FACS. For degradation of IgM molecules, serum was
incubated for 45 min with 20 mmol/l dithiotreitol (DTT; Sigma
Chemical Co., St Louis, MO, USA) and tested by ABO-FACS.
ABO-FACS
Undiluted serum (35 ll) was incubated with 25 ll of a 1%
solution of fixed RBC for 30 min at 4�C and subsequently
washed once in 3 ml of FACS buffer (0Æ1% BSA in Hank’s
buffered salt solution). Binding of anti-A/B Ab was measured
by indirect flow cytometry using secondary phcoerythrin-
labelled Ab (goat anti-human IgG; Zymed Laboratories, Inc.,
San Francisco, CA, USA; goat anti-human IgM; Sigma
Chemical Co.). A minimum of 10 000 events was acquired
on the flow cytometer. Human AB-serum from a single-donor
was further depleted of potentially autoreactive anti-A/B Ab by
incubation with highly concentrated A and B RBC and used as
negative control. To exclude binding of irregular RBC Ab, a
commercially available panel of O RBC expressing different
Rh, MNS, P, Lewis, Lutheran, Kell, Duffy, Kidd and sex-linked
RBC Ag was pooled and included into all assays (Screening test
for irregular RBC Ab; Reagent RBCs for antibody identifica-
tion, Gamma Biologicals, Inc., Houston, TX, USA). As positive
control human serum of a healthy donor of blood group O
with high anti-A/B Ab levels was included in all assays. Using
serially diluted sera, antibody binding, as measured by ABO-
FACS, was clearly dose dependent (data not shown). In
addition, each serum was incubated with fixed porcine RBC
because the serum of the majority of healthy individuals
contains xenoreactive natural Ab. To compare the levels of
anti-A/B Ab binding the geometric mean fluorescence intensity
ratios (MFIR) were calculated by dividing the mean fluores-
cence intensity of the sera of interest with the mean fluores-
cence intensity of the negative control. To validate the results,
all measurements were performed in two independent experi-
ments and displayed as mean values. Comparison of three
series of experiments yielded a good interassay correlation
(Spearman rs ¼ 0Æ945 between series 1 and 2; and rs ¼ 0Æ969between series 2 and 3 experiments, both P < 0Æ001).In 15 samples with high total IgG, IgG-subclass analysis was
performed using specific biotinylated secondary Ab for IgG1,
2, 3, and 4 (Zymed Laboratories, Inc.) and a streptavidin-
fluorescein isothiocyanate (FITC) conjugate (BD Biosciences,
Pharmingen, San Diego, CA, USA). The sera were incubated
with RBC for 30 min at 4�C and washed once with Hank’s
buffered saline. Biotinylated secondary Ab were added for
Detection of ABO Antibodies by Flow Cytometry
ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963 955
30 min at 4�C and washed twice thereafter. In a third step,
streptavidin-FITC was incubated for 30 min at 4�C and
washed twice. The samples were then measured by flow
cytometry and the results displayed as MFIR.
Haemagglutination
Anti-A/B and anti-porcine haemagglutination titres were
measured with a microplate haemagglutination assay (Craw-
ford et al, 1970). Serially diluted serum was incubated with a
1% suspension of RBC in 0Æ9% NaCl for 30 min at room
temperature in 96-well U-bottom plates (Nunclon Surface;
NUNC, Roskilde, Denmark). Thereafter, the plates were
centrifuged at 300 g for 2 min and placed in an upright
position for 10 min. As discussed by Crawford et al (1970),
haemagglutination was judged positive when the RBC
remained as a clot and did not run down the well of the
96-well plate. Titres were expressed as the highest dilution that
caused haemagglutination. All experiments were performed
twice; in cases of more than one titre difference, a third
experiment was performed, and the median value was taken
for further analysis.
ABO-ELISA
Enzyme-linked immunosorbent assays were used to detect
anti-A/B Ab as described previously (Rieben et al, 1991). In
brief, polystyrene microtitre plates (NUNC maxisorp, NUNC
A/S) were coated overnight at 4�C with synthetic A or B
trisaccharides coupled to polyacrylamide (Syntesome, Mos-
cow, Russia). Subsequently, the plates were washed thrice in
PBS containing 0Æ05% Tween 20 (Sigma Chemicals Co.).
Serum samples were diluted 1:40 in PBS containing 1% BSA
(Fluka Biochemicals) and 5% Tween 20 and incubated for
90 min at 37�C on a shaker. Binding of human anti-A/B IgM
and IgG to the coat antigen was detected by incubation with
mouse monoclonal anti-human IgG or IgM (clones HB43 and
HB57 from ATCC), followed by biotinylated goat anti-mouse
IgG1 (Southern Biotechnology Associates, Birmingham, AL,
USA) for 1 h at 37�C on a shaker and streptavidin-alkaline
phosphatase conjugate (Amersham, Bucks, UK) for 30 min at
37�C. As a chromogenic substrate 4-nitrophenyl phosphate
was used (Fluka Biochemicals), and optical density (OD)
values were read in an ELISA reader at 405 nm. A value of 0Æ35OD was chosen as cut-off. As internal standard, a serum with
high anti-A/B titres was included in the assay. All assays were
run in duplicates and the blank was subtracted from the mean
values of the duplicates.
Statistics
All statistical analyses were performed with the Statistical
Package for the Social Sciences (SPSS) software (SPSS for
Windows, version 11.0). The groups were compared by
Student’s t-test or nonparametric tests as appropriate. Stand-
ard deviation (SD) or range was used as an estimate of
variance. Spearman’s rank correlation test was performed for
comparison between haemagglutination, ABO-ELISA and
ABO-FACS assays. Sensitivity and specificity were analysed
by receiver operating characteristic curves (ROC). All reported
P-values are two-sided, and P < 0Æ05 was assumed to be
statistically significant.
Results
IgM and IgG anti-A/B antibodies in healthy blood donors
The ABO-FACS was established and validated with 120 sera of
healthy blood donors. Fig 1A demonstrates the cell size
visualised by flow cytometry on a linear scale. Porcine RBC
showed a second population in the range of 15–25% after
fixation, most probably representing microagglutinates. A
second population indicating microagglutinates was not seen
in human RBC. The somewhat larger range of the human RBC
population was attributed to cellular debris. Characteristic
results of the ABO-FACS for one donor of each blood group
are demonstrated in Fig 1B. As expected, anti-A IgM was
detected in the sera of blood group B and O, but not in the sera
of blood group A and AB. Conversely, anti-B IgM was detected
in the sera of blood group A and O, but not in the sera of
blood group B and AB. The sera shown were all positive for
anti-porcine IgM and negative for irregular RBC Ab. As
described below, IgM and IgG were considered to be positive if
the MFIR was greater than 3Æ7 and 2Æ0 respectively. Table I
shows the numbers and percentages of positive samples in the
four blood groups. Anti-porcine IgM were present in 112 of
120 samples (93%) and anti-porcine IgG in 103 of 120 samples
(86%), irrespective of the ABO-blood group of the donor. The
screening test for irregular RBC IgM was positive in 13/120
samples (11%) and negative for irregular RBC IgG in all
samples. If the screening test for irregular RBC Ab was positive,
unexpected binding to RBC expressing the self-ABO Ag was
considered to be false positive and these samples were excluded
from the specificity calculations below. In the majority of
samples the presence of anti-A/B IgG was restricted to blood
group O: anti-A and/or anti-B IgG were found in 34/38
samples (89%). In contrast, only 4/28 samples (14%) with
blood group A had anti-B IgG, 1/28 samples (4%) with blood
group B had anti-A IgG, and none of the samples with blood
group AB had anti-A or anti-B IgG. There was a considerable
variability in the level of both anti-A/B IgM and IgG in all
blood groups. The median anti-A/B MFIR levels for 28 A, 28 B,
38 O, and 26 AB sera are displayed in Fig 2. Blood group O
samples contained higher levels of anti-A IgG than anti-B IgG
(mean MFIR 9Æ2 vs. 3Æ8), corresponding to the higher number
of anti-A IgG positive samples when compared with the anti-B
IgG positive samples shown in Table I (76% vs. 66%). In 15
blood group O samples with high anti-A/B or anti-porcine IgG
levels, IgG subclass analysis was performed. As shown in Fig 3,
the predominant IgG subclass was IgG2. Low levels of IgG1
G. Stussi et al
956 ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963
and IgG3 were found in seven and four donors respectively.
IgG4 was negative in all samples measured.
Reverse blood group typing
To determine the optimal diagnostic cut-off level of the ABO-
FACS, ROC were calculated. This statistical procedure pro-
vides the sensitivity and 1-specificity for continuous variables,
such as the MFIR. The levels of anti-A/B IgM were compared
with conventional blood group typing and produced an
optimal sensitivity (93%) and specificity (96%) at an MFIR
cut-off level of 3Æ7 (Fig 4). The area under the curve (AUC) of
the ROC analysis was 0Æ972 [n ¼ 214; 95% confidence interval
(CI), 0Æ951–0Æ993; P < 0Æ001], indicating a high accuracy of
anti-A/B IgM to predict the correct blood group. In contrast,
anti-A/B IgG FACS values were not useful for reverse blood
group typing. The mean levels of anti-A and anti-B IgG MFIR
in blood group B and A sera were 1Æ5 and 1Æ2 respectively.
Meaningful calculations of the sensitivity could only be
obtained at an MFIR cut-off level of 2Æ0. Using this cut-off
level, the presence of anti A/B IgG was highly specific for blood
group O samples (data not shown).
Comparison of ABO-FACS with haemagglutination
The MFIR levels of anti-A/B Ab as determined by ABO-FACS
were compared with the anti-A/B Ab titres obtained by
microplate haemagglutination assays in 120 sera. As shown in
Fig 5, an overall correlation coefficient of 0Æ870 for IgM and
0Æ783 for IgG was obtained by Spearman’s rank testing. The
correlation between anti-A IgM MFIR and anti-A haemagglu-
tination titre was 0Æ862 and between anti-B IgM MFIR and
anti-B haemagglutination titre 0Æ880. Eight samples with
negative haemagglutination titres were positive for anti-A/B
IgM in the ABO-FACS, but five of these eight samples were
also positive in the screening test for non-ABO anti-RBC Ab.
Thus, overall, only 3/82 samples (4%) of blood group A, B, or
AB were positive in the ABO-FACS and negative in the
haemagglutination assay, indicating the occurrence of anti-A/B
Ab that bind to RBC but do not induce haemagglutination. On
the contrary, 6/94 samples (6%) of blood group A, B, or O
expressed low haemagglutination titres (range: 1:2–1:32), while
the anti-A/B IgM MFIR was below the cut-off level. These
ABO-FACS results were therefore considered to be false
negative. This finding indicated that in some cases low
A B O AB
Cel
l nu
mb
er
Mean fluorescence intensity(logarithmic scale)
Anti-Scr
101 102 103 101 102 103 101 102 103 101 102 103
1·0 1·3 1·3
14·5 26·2 15·4
Anti-Pig
6·2
Anti-A
Anti-B
1·1
25·7
18·7
1·3
14·2
9·8
1·1
1·5
1·2
Donor blood group
Mean fluorescence intensity(linear scale)
A
B
Po RBC
SS
C
FSC
Human RBC
SS
C
FSC
21%
Fig 1. (A) Density plots of porcine (Po) and human RBC incubated
with human serum derived from a blood group O donor. The cell size
was visualised by FACS on a linear scale, the X-axis represents the size
of the cells by forward scatter (FSC) measurement, the Y-axis repre-
sents the granularity of the cells by sideward scatter (SSC) measure-
ment. (B) Measurement of anti-A/B IgM by ABO-FACS: the anti-A/B
IgM MFIR levels were determined by ABO-FACS in sera of blood
donors of blood group A, B, O, and AB, respectively. The X-axis
represents the mean fluorescence intensity (logarithmic scale), the
Y-axis the cell number. Open histograms represent the staining with
absorbed human AB serum for human RBC and porcine serum for
porcine RBC (negative control). The filled histograms represent
binding of IgM Ab present in the tested serum to blood group A (anti-
A), B (anti-B), porcine (anti-Pig), or screening RBC for irregular RBC
Ab (anti-Scr). Anti-porcine IgM (positive control) were present in all
four sera, whereas the screening test for irregular RBC Ag (anti-Scr)
was negative in all four sera. Numbers indicate mean fluorescence
intensity ratios (MFIR), for calculation see Materials and Methods.
Table I. Frequency of anti-A/B and anti-porcine antibodies.
Blood group
A B O AB Total
Number 28 28 38 26 120
IgM antibodies [n (%)]
Anti-A IgM* 1 (4) 26 (93) 36 (95) 1 (4) 64 (53)
Anti-B IgM* 26 (93) 0 36 (95) 1 (4) 63 (52)
Anti-Po IgM 27 (96) 25 (89) 35 (92) 25 (96) 112 (93)
Screening IgM 4 (14) 3 (11) 4 (11) 2 (8) 13 (11)
IgG antibodies [n (%)]
Anti-A IgG 0 4 (14) 29 (76) 0 33 (28)
Anti-B IgG 1 (4) 0 25 (66) 0 26 (22)
Anti-Po IgG 27 (96) 22 (79) 38 (100) 16 (61) 103 (86)
Screening IgG 0 0 0 0 0
*If the screening test for irregular RBC Ab was positive, sera were not
included into the analysis.
Detection of ABO Antibodies by Flow Cytometry
ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963 957
concentrations of anti-A/B Ab are able to induce haemagglu-
tination, whereas Ab-independent haemagglutination is rather
unlikely.
ABO-ELISA in comparison with haemagglutination andABO-FACS
Another method to measure anti-A/B Ig isotypes is the ABO-
ELISA using synthetic A and B trisaccharides coupled to
polyacrylamide as coating substance. The anti-A/B Ab MFIR
levels obtained by ABO-FACS were compared with the OD
levels of the ABO-ELISA. For this purpose, 29 serum samples
of blood group A (9), B (6), O (12), and AB (2) were randomly
chosen. Spearman’s rank correlation of the ABO-ELISA with
the ABO-FACS assay was 0Æ654 for anti-A/B IgM and 0Æ684 foranti-A/B IgG. Correlation between ABO-ELISA and haemag-
glutination yielded an overall correlation of 0Æ550 for anti-A/B
IgM and 0Æ513 for anti-A/B IgG. Furthermore, a ROC curve
IgM
IgG
A (n = 28) B (n = 28) O (n = 38) AB (n = 26)
Donor blood group
Anti-A/B/pig antibodies
A B Pig A B Pig A B Pig A B Pig
0
50
100
150
0
10
20
30
40MF
IR
Fig 2. Levels of anti-A/B antibodies in the sera of 120 healthy blood donors: Anti-A/B IgM and IgG levels were measured in the sera of 120 healthy
blood donors, 28 A, 28 B, 38 O, and 26 AB respectively. The box plots show the median MFIR values and the 25th and 75th percentiles, the whiskers
represent the 95% confidence intervals. Open box plots represent anti-A Ab, light grey box plots anti-B and dark grey box plots anti-porcine (Pig)
antibodies. The upper panel shows the results of IgM measurements, the lower panel IgG.
0
5
10
15
IgG1 IgG2 IgG3 IgG4
P < 0·001
MF
IR
Fig 3. Anti-A/B IgG subclass analysis in sera of 15 blood group O
donors: IgG subclasses were analysed by ABO-FACS in 15 blood group
O donors with high anti-A/B IgG levels. The bars represent mean
values (+SD). All six 15 donors were positive for the IgG2 subclass,
whereas seven donors were positive for IgG1 and four donors for IgG3.
IgG4 was negative in all samples. The differences among the four
subclasses were statistically significant using a Kruskal-Wallis test as
indicated by the P-value. The detection limit (MFIR ¼ 1) is indicated
with a horizontal line.
1-specificity
Sen
siti
vity
10·750·500·25
1
0·75
0·50
0·25
AUC 0·972, P < 0·001
Fig 4. ROC curve analysis to determine sensitivity and specificity of
the ABO-FACS: ROC curve analysis was used to determine the optimal
sensitivity and specificity of the continuous MFIR data obtained by
ABO-FACS. The area under the curve (AUC) indicates the accuracy of
the assay. Comparison between anti-A/B IgM MFIR levels and the
effective ABO blood group as determined by conventional forward
blood group typing yielded a 96% specificity and 93% sensitivity at a
cut-off level of 3Æ7. The AUC was 0Æ972 (95% confidence interval
0Æ951–0Æ993, P < 0Æ001).
G. Stussi et al
958 ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963
analysis was performed to determine the cut-off level for
optimal sensitivity and specificity of the ABO-ELISA to detect
the correct blood group. At a value of 0Æ35 OD the sensitivity
and specificity were 62% and 63%, respectively (AUC 0Æ675,95% CI 0Æ5270–0Æ823; P ¼ 0Æ032). Anti-A/B IgM against self-
ABO Ag were detected in as many as 7/17 samples (41%) with
blood group A, B, or AB. The haemagglutination titre was
negative in all cases, whereas one of these seven samples
yielded a positive ABO-FACS result. However, this sample
could be considered a false positive result, because the
screening test for non-ABO RBC Ab was also positive. Three
of 17 samples (18%) were positive for anti-A/B IgG against
self-ABO Ag in the ABO ELISA, whereas autoreactive anti-A/B
IgG were not detectable in blood group A, B and AB samples
by ABO-FACS (Table I). According to the low sensitivity of
the ABO-ELISA obtained by ROC analysis a high number of
false negative results were observed. Anti-A/B IgM was below
the cut-off level of the ABO-ELISA in 12/27 samples (44%) of
blood group A, B, or O, all of which had positive haemag-
glutination titres. In one sample anti-A IgM was negative in
both ABO-ELISA and ABO-FACS, but showed low-level
haemagglutination (1:2).
Comparison of ABO-FACS with standard methods todetermine anti-A/B IgG
In clinical routine, anti-A/B IgG is determined by addition of
DTT to the serum followed by a crosslinking anti-IgG Ab
(indirect Coombs assay). Therefore, the effect of DTT on the
MFIR levels of IgM and IgG as determined by ABO-FACS was
analysed by the incubation of four sera with DTT. At a
concentration of 20 mmol/l, DTT predominantly degraded
IgM by reduction of intermolecular disulphide bonds, whereas
the intramolecular disulphide bonds of IgG were only affected
at higher concentrations. As shown in Fig 6A, DTT completely
abrogated the binding of IgM to the RBC, whereas IgG binding
was only slightly reduced by DTT, suggesting a minimal
destruction of IgG molecules. Another technique often applied
to discriminate IgG from IgM is the use of differential binding
qualities of IgM and IgG Ab at 4�C and 37�C. As displayed in
Fig 6B, overall binding of anti-A/B IgM as well as IgG was
higher at 4�C than at room temperature or 37�C. These data
seemed to confirm the usefulness of DTT to determine the
presence of IgG antibodies in a functional assay, whereas the
temperature method did not seem to be appropriate.
Cross-reactive anti-A/B antibodies
In the final series of experiments we studied whether Ab cross-
reacted to A and B Ag. For this purpose, seven blood group O
sera were absorbed with either O, A, or B RBC prior to ABO-
FACS analysis. After absorption, there was a 8%, 100% and
17% mean reduction of anti-A IgM, respectively, and a 7%,
33% and 100% mean reduction of anti-B IgM respectively
(Fig 7, upper panel). Similarly, there was a 3%, 100% and
18%, mean reduction of anti-A IgG, and a 4%, 18% and 100%
mean reduction of anti-B IgG MFIR levels after absorption
(Fig 7, lower panel). As expected, anti-A and anti-B Ab were
completely removed from blood group O sera by absorption
with A or B RBC, respectively. In contrast, absorption with A
RBC also reduced anti-B MFIR levels by a mean of 17% (0–
39%) and incubation with B RBC reduced anti-A MFIR levels
by a mean 33% (0–89%). This suggested the presence of cross-
reactive IgM in some of the O donors. This finding was specific
for blood group O sera, as absorption of blood group A sera
with A RBC did not change the level of anti-B IgM. The anti-B
IgM present in blood group A sera was completely removed by
incubation with B RBC. Conversely, incubation of blood group
B sera with A RBC almost completely reduced the anti-A IgM
levels whereas incubation with B RBC did not alter anti-A IgM
levels (data not shown).
Discussion
This study has shown that the ABO-FACS is a valid tool to
quantify the binding of anti-A/B Ab to human RBC. As
compared with classical functional assays, such as tube
haemagglutination and indirect antiglobulin testing, and a
previously described ABO-ELISA, the ABO-FACS offers several
advantages: First, it measures the presence of all anti-A/B Ab
binding to the respective ABO Ag expressed on RBC, not only
haemagglutinating or haemolysing Ab. Secondly, binding of
anti-A/B Ab to natural ABO Ag on RBC was clearly more
sensitive and more specific than binding to synthetic ABO Ag
immobilised on ABO-ELISA plates. Thirdly, the ABO-FACS
directly quantifies the binding of different anti-A/B Ab isotypes
and IgG subclasses using specific secondary Ab. For these
reasons the ABO-FACS offers a novel high throughput and
Agglutination (1/x)
MF
IR (
log
arit
hm
ic s
cale
)
0·1
1
10
100
1000
0 1 2 4 8 16 32 64 128 256 512 1024
MFIR 3·7
r = 0·870, P < 0·001
Fig 5. Correlation between ABO-FACS and haemagglutination: MFIR
values obtained by ABO-FACS (Y-axis) and haemagglutination titres
(X-axis) in all 120 tested sera are shown using logarithmic scales. The
overall correlation as calculated by Spearman’s rank testing yielded a
coefficient of 0Æ870 (P < 0Æ001). The cut-off level of the IgM ABO-
FACS (MFIR ¼ 3Æ7) is indicated with a horizontal line.
Detection of ABO Antibodies by Flow Cytometry
ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963 959
observer-independent method that can be used to monitor
anti-A/B Ab levels in large studies and to validate other
techniques.
Technically, the ABO-FACS analysis could be hampered by
RBC aggregates in the presence of haemagglutinating Ab.
Fixation of RBC with formaldehyde and glutaraldehyde
(Karnovsky buffer) largely prevented haemagglutination. A
subpopulation of microagglutinates consisting of two RBC was
observed using fixed porcine RBC, but not with human RBC of
blood group A or B. However, the flow cytometric analysis
using a logarithmic scale was not hampered by these micro-
agglutinates. Other flow cytometry studies to measure anti-A/B
Ab applied vacuum filtration or centrifugation over a filter
membrane to disperse RBC in an attempt to obtain single-cell
suspensions (Roback et al, 2003, 2004).
Although the exact mechanism leading to inhibition of
agglutination by fixation is unknown, cross-linking of proteins
stabilises RBC membranes and thereby impairs lateral move-
ments of ABO Ag, which is required for efficient haemagglu-
tination. Theoretically, fixation with Karnovsky buffer might
also result in structural alterations of RBC epitopes, including
ABO Ag, and thereby might change the anti-A/B Ab binding
pattern. In the current analysis we did not have any evidence
that the specificity or density of ABO Ag was transformed,
changes in the expression of other RBC Ag however cannot be
ruled out. Although Berneman et al (1991) reported that
formaldehyde fixation reduces the total number of ABO Ag on
RBC, we did not detect major differences of anti-A/B Ab levels
using RBC of several donors and after serial fixations with
Karnovsky buffer. Thus, the ABO Ag density was relatively
constant after fixation with Karnovsky buffer (data not shown).
Nonetheless, to minimise potential differences, we stored large
batches of single donor RBC in liquid nitrogen following shock
freezing, which can be used for ABO-FACS up to 6 weeks after
thawing and fixation without deterioration of the Ab binding.
Cel
l nu
mb
er
Negative control
30 min, 4°C
30 min, 37°C
Temperature
IgM IgG
MF
IR
IgMA BIgG
0
10
20
30
40
50
+0
5
10
15
20
25
30
DTT treatment
Negative control
Native serum
DTT treatment
+
IgM/G MFI (logarithmic scale) IgM/G MFI (logarithmic scale)
MF
IRC
ell n
um
ber
0
10
20
30
40
50
4°C RT 37°C0
5
10
15
20
25
4°C RT 37°C
Fig 6. Effect of dithiotreitol (DTT) and temperature on anti-A/B Ab binding: (A) Measurements of anti-A/B IgM (left panel) and IgG (right panel)
by ABO-FACS following incubation of the serum with DTT. The upper panel shows a representative binding of anti-A/B Ab with (light grey
histograms) or without DTT treatment (dark grey histograms), and staining with absorbed human AB serum as negative control (open histograms).
The lower panel summarises the effect of DTT on anti-A/B IgM MFIR values in four sera (left panel) and anti-A/B IgG MFIR values in three sera
(right panel) respectively. The figure represents one of two independent experiments. (B) Measurements of anti-A/B IgM (left panel) and IgG (right
panel) by ABO-FACS performed at 4�C, room temperature and 37�C respectively. The filled histograms represent binding of anti-A/B Ab at 37�C(light grey) or at 4�C (dark grey). The lower panel summarises the temperature effect on anti-A/B IgM MFIR values (left panel) and anti-A/B IgG
MFIR values (right panel) in seven sera respectively. The figure represents one of five independent experiments.
0
20
40
60
80
100
Anti-A
0
20
40
60
80
100
0
20
40
60
80
100
Anti-B
0
20
40
60
80
100
Red blood cells used for absorption
% M
FIR
(u
nab
sorb
ed c
on
tro
l ser
um
)
IgM
IgG
O A B O A B
O A B O A B
Fig 7. Evidence for the presence of cross-reactive anti-A/B Ab in blood
group O sera: blood group O sera were incubated with RBC and
analysed for the presence of anti-A/B IgM (upper panel) and anti-A/B
IgG (lower panel) by ABO-FACS. The bars represent relative mean
MFIR ± SD of anti-A (left panel) and anti-B (right panel) Ab binding
after absorption with blood group O (open), A (grey), or B RBC
(black) relative to the anti-A/B Ab MFIR of unabsorbed serum. The
data shown are pooled from four independent experiments repre-
senting seven blood group O sera.
G. Stussi et al
960 ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963
Controversial results have been reported on the measure-
ment of anti-A/B IgG and IgG subclasses by gel tests, ELISA,
immunofluorescence and flow cytometry (Owen, 1954; Raw-
son & Abelson, 1960; Kay & Locke, 1986; Brouwers et al, 1987;
Rieben et al, 1991; Lynen et al, 1995; Fabijanska-Mitek et al,
1997). Our data with FACS analysis on IgG subclasses in 15
samples with high anti-A/B IgG Ab revealed a predominance of
IgG2 Ab. IgG1 and IgG3 were found only in seven and four
donors, respectively, and IgG4 was not detectable. These
findings are in line with the results of some earlier studies, but
contrast with others (Kay & Locke, 1986; Brouwers et al, 1987;
Fabijanska-Mitek et al, 1997), thereby reflecting methodologi-
cal problems, such as the choice of the antigenic source, the
specificity of secondary Ab and the sensitivity of the detection
system. Although we cannot draw a final conclusion on the
distribution of IgG subclasses from analysing 15 samples, the
ABO-FACS avoids many of the technical problems that
hampered previously used methods. In addition, it parallels
the situation of other bacterial polysaccharides predominantly
evoking IgG2 subclass responses. Although it is still contro-
versial whether IgG2 subclass deficiency is associated with a
higher incidence of bacterial infections, it has been shown in
numerous studies that IgG2 are highly active against bacterial
polysaccharides (Siber et al, 1980; Maguire et al, 2002).
Moreover, differentiation between IgM and IgG Ab is difficult
to achieve by using standard techniques and depends on
surrogate procedures, such as performance at different tem-
peratures or after dissociation of IgM molecules by reducing
agents. We could confirm that IgM generally binds more avidly
at 4�C, however, more importantly, that binding of anti-A/B
IgG was also reduced at room temperature and 37�C in several
samples. Thus, mere differentiation of IgM and IgG by
temperature seems inappropriate. In contrast, the DTT
treatment seemed suitable for the determination of anti-A/B
IgG.
Cross-reactive anti-A/B Ab binding to both A and B Ag,
have been demonstrated by several groups, especially after
immunisation with A and B Ag (Owen, 1954; Holburn, 1976;
Contreras et al, 1984). In the present study, we provide
indirect evidence for the occurrence of cross-reactive anti-A/B
Ab in the sera of some, but not all O donors. In contrast, cross-
reactive Ab were not detected in the sera of blood group A or
B, presumably because subjects with blood group O lack the
selective pressure to eliminate B-lymphocytes producing cross-
reactive anti-A/B Ab.
Comparison of ABO-FACS MFIR values and haemaggluti-
nation titres showed good correlation between the two assays
and the measurement of anti-A/B IgM by ABO-FACS enabled
the correct prediction of the blood group (reverse typing) in
the majority of the samples. These findings indicate that the
majority of anti-A/B IgM are haemagglutinating Ab. On the
contrary, the correlation between ABO-ELISA and ABO-FACS
was weak, as was the correlation between ABO-ELISA and
haemagglutination, even lower than originally reported (Rie-
ben et al, 1991). In the current study, a high number of
samples containing potentially autoreactive Ab was found by
ABO-ELISA (41% IgM, 18% IgG), but not by ABO-FACS (4%
IgM, 0% IgG). These findings might be explained by the use of
synthetic ABO Ag in the ABO-ELISA, which exhibit an
incomplete antigenic structure and are bound to a carrier
substance, such as polyacrylamide or BSA. Binding of
low-affinity and low-specificity Ab may have potentially
overestimated the levels of anti-A/B Ab and the presence of
auto-reactive Ab (Rieben et al, 1991). In addition, the
screening test for non-ABO RBC Ab can identify false positive
samples in the ABO-FACS and increases thereby the accuracy
of the ABO-FACS assay. Thus, using the ABO-FACS, the
incidence of autoreactive anti-A/B Ab is lower than expected
from the results obtained by the ABO-ELISA.
In contrast to anti-A/B IgM, ‘immune’ anti-A/B IgG are
predominantly found in blood group O sera or after immu-
nisation with the respective ABO Ag (Rawson & Abelson, 1960;
Contreras et al, 1984). In fact, the present study revealed anti-
A/B IgG by ABO-FACS in 89% of the blood group O samples,
but only in 6% of non-O sera, a value similar to that found
earlier (Rawson & Abelson, 1960; Kay & Locke, 1986). To date,
there is no explanation for the latter finding, but low anti-A in
B and low anti-B in A may provide an advantage to women
with these blood groups during ABO incompatible pregnan-
cies, because only IgG are transferred through the placenta,
exposing the child to the risk of haemolytic disease. This view
is supported by the clinical finding, that only newborns of
blood group O mothers develop haemolytic disease after ABO-
incompatible pregnancies (Brouwers et al, 1988). The apparent
lack of antibody class switch in blood group A and B
individuals may represent an interesting in vivo model to
study the development of the natural Ab repertoire.
Beside the ABO-FACS reported here, another elegant
method quantifying anti-A/B IgM and IgG by surface plasmon
resonance was recently reported (Kimura et al, 2005). This
method measures changes of the physical properties of Ab/
ABO Ag complexes of which the latter are immobilised to a
sensor chip. The classical tube haemagglutination assay
remains the gold standard in clinical routine. However, novel
methods to determine anti-A/B Ab levels are being developed
to closely monitor these Ab in different clinical settings, such
as ABO-incompatible transplantations, providing an excellent
model to study humoral immune responses in vivo. Accidental
ABO incompatibility in solid organ transplantation usually
results in catastrophic hyperacute rejection because of the
expression of ABO Ag on graft endothelial cells (Cooper,
1990). Nevertheless, sophisticated protocols have allowed
ABO-incompatible living donor kidney and liver transplanta-
tions (Cacciarelli et al, 1995; Takahashi et al, 2004; Winters
et al, 2004; Tyden et al, 2005). The importance of anti-A/B Ab
measurements in these settings is stressed by the fact that high
pretransplant anti-A/B IgG haemagglutination titres were
associated with poor graft survival, irrespective of pretrans-
plant procedures to lower these Ab titres (Shimmura et al,
2000). Interestingly, ABO-mismatched haematopoietic stem
Detection of ABO Antibodies by Flow Cytometry
ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963 961
cell transplantation does not influence the patient’s outcome
(Hershko et al, 1980; Bensinger et al, 1982; Kalaycioglu et al,
1995; Seebach et al, 2005), presumably because of regulatory
processes on the level of Ab production reported both after
incompatible solid organ and haematopoietic stem cell trans-
plantations (Mohiuddin et al, 2003; Takahashi, 2004). Alter-
natively, incompatible Ab may completely disappear after
transplantation, as found in both ABO-incompatible HSCT
(Stussi et al, 2005) and neonatal ABO-incompatible heart
transplantations (West et al, 2001; Fan et al, 2004).
In conclusion, we developed a sensitive and accurate
method to quantify the concentrations of anti-A/B Ab as
well as IgG subclasses by means of flow cytometry. While
this work has focused on anti-A/B Ab levels in healthy blood
donors, it is suitable to study anti-A/B Ab in clinical
situations, such as ABO-incompatible HSCT, solid organ
transplantation and haemolytic disease of the newborn. In
ABO-incompatible solid organ and stem cell transplantation,
accurate measurements of ABO antibodies will give insights
into the immunological mechanisms leading to the graft
acceptance including antibody class switch, accommodation
and tolerance induction. Moreover, analysing anti-A/B Ab
levels prior ABO-incompatible kidney transplantation can
identify patients suitable for ABO-incompatible kidney
transplantations and post-transplant monitoring can identify
those patients at risk for humoral rejection. In mothers with
ABO-incompatible pregnancies, the assay can be used to
detect stimulation of the maternal immune system due to
the ABO-incompatible fetal Ag during pregnancy or at
delivery. Finally, this current method can be applied for the
monitoring of removal of A and B Ag from RBC by enzyme
degradation.
Acknowledgements
This work was supported by grants from the Swiss National
Science Foundation (4046-058668/1) and the Julius-Muller
Stiftung to J.D.S. and a grant from the Heuberg Stiftung to
G.S. The authors thank Katja Matozan for performing the
ABO-ELISA experiments and the local transfusion service for
providing the serum and RBC samples. Dr F. Salomon is
acknowledged for critical reading of the manuscript and
helpful discussions.
References
Avrameas, S. (1991) Natural autoantibodies: from ‘horror autotoxicus’
to ‘gnothi seauton’. Immunology Today, 12, 154–159.
Bar, B.M., Schattenberg, A., Van Djik, B.A., De Man, A.J., Kunst, V.A.
& De Witte, T. (1995) Erythrocyte repopulation after major ABO
incompatible transplantation with lymphocyte-depleted bone mar-
row. Bone Marrow Transplantation, 16, 793–799.
Bensinger, W.I., Buckner, C.D., Thomas, E.D. & Clift, R.A. (1982)
ABO-incompatible marrow transplants. Transplantation, 33, 427–
429.
Berneman, Z.N., van Bockstaele, D.R., Uyttenbroeck, W.M., Van
Zaelen, C., Cole-Dergent, J., Muylle, L. & Peetermans, M.E. (1991)
Flow-cytometric analysis of erythrocytic blood group A antigen
density profile. Vox Sanguinis, 61, 265–274.
Brecher, M.E. (2002) American Association of Blood Banks, Technical
manual, 14th edn. American Association of Blood Banks, Bethesda.
Brouwers, H.A., Overbeeke, M.A., Gemke, R.J., Maas, C.J., van Leeu-
wen, E.F. & Engelfriet, C.P. (1987) Sensitive methods for
determining subclasses of IgG anti-A and anti-B in sera of blood-
group-O women with a blood-group-A or -B child. British Journal of
Haematology, 66, 267–270.
Brouwers, H.A., Overbeeke, M.A., van Ertbruggen, I., Schaasberg, W.,
Alsbach, G.P., van der Heiden, C., van Leeuwen, E.F., Stoop, J.W. &
Engelfriet, C.P. (1988) What is the best predictor of the severity of
ABO-haemolytic disease of the newborn? Lancet, 2, 641–644.
Buchs, J.P. & Nydegger, U.E. (1989) Development of an ABO-ELISA
for the quantitation of human blood group anti-A and anti-B IgM
and IgG antibodies. Journal of Immunological Methods, 118, 37–46.
Cacciarelli, T.V., So, S.K., Lim, J., Concepcion, W., Cox, K. & Esquivel,
C.O. (1995) A reassessment of ABO incompatibility in pediatric liver
transplantation. Transplantation, 60, 757–760.
Contreras, M., Armitage, S.E. & Hewitt, P.E. (1984) Response to
immunization with A and B human glycoproteins for the procure-
ment of blood grouping reagents. Vox Sanguinis, 47, 224–235.
Cooper, D.K. (1990) Clinical survey of heart transplantation between
ABO blood group-incompatible recipients and donors. Journal of
Heart Transplantation, 9, 376–381.
Coutinho, A., Kazatchkine, M.D. & Avrameas, S. (1995) Natural
autoantibodies. Current Opinion in Immunology, 7, 812–818.
Crawford, M.N., Gottman, F.E. & Gottman, C.A. (1970) Microplate
system for routine use in blood bank laboratories. Transfusion, 10,
258–263.
Fabijanska-Mitek, J., Lopienska, H. & Zupanska, B. (1997) Gel test
application for IgG subclass detection in auto-immune haemolytic
anaemia. Vox Sanguinis, 72, 233–237.
Fan, X., Ang, A., Pollock-Barziv, S.M., Dipchand, A.I., Ruiz, P.,
Wilson, G., Platt, J.L. & West, L.J. (2004) Donor-specific B-cell
tolerance after ABO-incompatible infant heart transplantation.
Nature Medicine, 10, 1227–1233.
Hershko, C., Gale, R.P., Ho, W. & Fitchen, J. (1980) ABH antigens and
bone marrow transplantation. British Journal of Haematology, 44,
65–73.
Holburn, A.M. (1976) Radioimmunoassay studies of the cross-reacting
antibody of human group O sera. British Journal of Haematology, 32,
589–599.
Kalaycioglu, M., Copelan, E., Avalos, B., Klein, J., Goormastic, M. &
Bolwell, B. (1995) Survival after ABO-incompatible allogeneic bone
marrow transplant after a preparative regimen of busulfan and
cyclophosphamide. Bone Marrow Transplantation, 15, 105–110.
Kay, L.A. & Locke, D. (1986) Distribution of immunoglobulin G
subclasses in anti-A and anti-B sera. Journal of Clinical Pathology, 39,
684–687.
Kimura, S., Yurugi, K., Segawa, H., Kuroda, J., Sato, K., Nogawa, M.,
Yuasa, T., Egawa, H., Tanaka, K. & Maekawa, T. (2005) Rapid
quantitation of immunoglobulin G antibodies specific for blood
group antigens A and B by surface plasmon resonance. Transfusion,
45, 56–62.
Landsteiner, K. (1901) Ueber Agglutinationserscheinungen normalen
menschlichen Blutes. Wiener klinische Wochenschrift, 14, 1132–1134.
G. Stussi et al
962 ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963
Lutz, H.U. (2004) Innate immune and non-immune mediators of
erythrocyte clearance. Cellular and Molecular Biology, 50, 107–116.
Lutz, H.U., Fasler, S., Stammler, P., Bussolino, F. & Arese, P. (1988)
Naturally occurring anti-band 3 antibodies and complement in
phagocytosis of oxidatively stressed and in clearance of senescent red
cells. Blood Cells, 14, 175–203.
Lynen, R., Neuhaus, R., Schwarz, D.W., Simson, G., Riggert, J., Mayr,
W.R. & Kohler, M. (1995) Flow cytometric analyses of the subclasses
of red cell IgG antibodies. Vox Sanguinis, 69, 126–130.
Maguire, G.A., Kumararatne, D.S. & Joyce, H.J. (2002) Are there any
clinical indications for measuring IgG subclasses? Annals of Clinical
Biochemistry, 39, 374–377.
Mohiuddin, M.M., Ogawa, H., Yin, D.P., Shen, J. & Galili, U. (2003)
Antibody-mediated accommodation of heart grafts expressing an
incompatible carbohydrate antigen. Transplantation, 75, 258–262.
Nussbaumer, W., Schwaighofer, H., Gratwohl, A., Kilga, S., Schonitzer,
D.,Nachbaur,D.&Niederwieser,D. (1995)Transfusionofdonor-type
red cells as a single preparative treatment for bonemarrow transplants
with major ABO incompatibility. Transfusion, 35, 592–595.
Owen, R. (1954) Heterogeneity of antibodies to the human blood
groups in normal and immune sera. Journal of Immunology, 73,
29–39.
Pins, M.R., Saidman, S.L., Cosimi, A.B., Jennings, L.D. & Stowell, C.P.
(1997) Accelerated acute rejection of an apparent A2 renal allograft
in an O recipient: report of a case with flow cytometric analysis.
Transplantation, 63, 984–988.
Rawson, A. & Abelson, N. (1960) Studies of blood group antibodies.
IV. Physicochemical differences between isoanti-A, B and isoanti-A
or isoanti-B. Journal of Immunology, 85, 640–647.
Rieben, R., Buchs, J.P., Fluckiger, E. & Nydegger, U.E. (1991) Anti-
bodies to histo-blood group substances A and B: agglutination titers,
Ig class, and IgG subclasses in healthy persons of different age
categories. Transfusion, 31, 607–615.
Roback, J.D., Barclay, S. & Hillyer, C.D. (2003) An automatable format
for accurate immunohematology testing by flow cytometry. Trans-
fusion, 43, 918–927.
Roback, J.D., Barclay, S. & Hillyer, C.D. (2004) Improved method for
fluorescence cytometric immunohematology testing. Transfusion,
44, 187–196.
Rydberg, L. (2001) ABO-incompatibility in solid organ transplanta-
tion. Transfusion Medicine, 11, 325–342.
Seebach, J.D., Stussi, G., Passweg, J.R., Loberiza, F.R., Ilhan, O.,
Gajewski, J.L., Keating, A., Goerner, M., Rowlings, P.A., Thibergien,
P., Elfenbein, G.J., Gale, R.P., van Rood, J.J., Reddy, V., Gluckman,
E., Bolwell, B.J., Klumpp, T.R., Horowitz, M.M., Ringden, O. &
Barrett, A.J. (2005) ABO blood group barrier in allogeneic hema-
topoietic stem cell transplantation revisited. Biology of Bone and
Marrow Transplantation, in press.
Shimmura, H., Tanabe, K., Ishikawa, N., Tokumoto, T., Takahashi, K.
& Toma, H. (2000) Role of anti-A/B antibody titers in results of
ABO-incompatible kidney transplantation. Transplantation, 70,
1331–1335.
Siber, G.R., Schur, P.H., Aisenberg, A.C., Weitzman, S.A. & Schiffman,
G. (1980) Correlation between serum IgG-2 concentrations and the
antibody response to bacterial polysaccharide antigens. New England
Journal of Medicine, 303, 178–182.
Sniecinski, I.J., Oien, L., Petz, L.D. & Blume, K.G. (1988)
Immunohematologic consequences of major ABO-mismatched
bone marrow transplantation. Transplantation, 45, 530–534.
Springer, G.F. & Horton, R.E. (1969) Blood group isoantibody sti-
mulation in man by feeding blood group-active bacteria. Journal of
Clinical Investigation, 48, 1280–1291.
Stussi, G., Huggel, K., Schanz, U., Passweg, J.R. & Seebach, J.D. (2005)
Levels of anti-A/B antibodies after ABO-incompatible hematopoietic
stem cell transplantation. Transplantation Proceedings, 37, 1385–
1387.
Takahashi, K. (2004) Accommodation in ABO-incompatible kidney
transplantation: why do kidney grafts survive? Transplantation
Proceedings, 36, 193S–196S.
Takahashi, K., Saito, K., Takahara, S., Okuyama, A., Tanabe, K., Toma,
H., Uchida, K., Hasegawa, A., Yoshimura, N. & Kamiryo, Y. (2004)
Excellent long-term outcome of ABO-incompatible living donor
kidney transplantation in Japan. American Journal of Transplanta-
tion, 4, 1089–1096.
Thompson, K.M., Sutherland, J., Barden, G., Melamed, M.D., Wright,
M.G., Bailey, S. & Thorpe, S.J. (1992) Human monoclonal anti-
bodies specific for blood group antigens demonstrate multispecific
properties characteristic of natural autoantibodies. Immunology, 76,
146–157.
Thorpe, S.J. & Bailey, S.W. (1993) Demonstration of autoreactivity by
a human monoclonal IgG anti-Rh D antibody. British Journal of
Haematology, 83, 311–318.
Tyden, G., Kumlien, G., Genberg, H., Sandberg, J., Lundgren, T. &
Fehrman, I. (2005) ABO incompatible kidney transplantations
without splenectomy, using antigen-specific immunoadsorption and
rituximab. American Journal of Transplantation, 5, 145–148.
Watkins, W.M. (2001) The ABO blood group system: historical
background. Transfusion Medicine, 11, 243–265.
West, L.J., Pollock-Barziv, S.M., Dipchand, A.I., Lee, K.J., Cardella,
C.J., Benson, L.N., Rebeyka, I.M. & Coles, J.G. (2001) ABO-in-
compatible heart transplantation in infants. New England Journal of
Medicine, 344, 793–800.
Winters, J.L., Gloor, J.M., Pineda, A.A., Stegall, M.D. & Moore, S.B.
(2004) Plasma exchange conditioning for ABO-incompatible renal
transplantation. Journal of Clinical Apheresis, 19, 79–85.
Detection of ABO Antibodies by Flow Cytometry
ª 2005 Blackwell Publishing Ltd, British Journal of Haematology, 130, 954–963 963