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Clinical Immunology 1
Defective tumor necrosis factor alpha-induced maturation of
monocyte-derived dendritic cells in patients with
myelodysplastic syndromes
Ilina Micheva*, Eleni Thanopoulou, Sotiria Michalopoulou, Marina Karakantza,
Alexandra Kouraklis-Symeonidis, Athanasia Mouzaki, Nicholas Zoumbos
Hematology Division, Department of Internal Medicine, Medical School and University Hospital, University of Patras, Patras, Greece
Received 29 June 2004; accepted 10 August 2004
Available online 18 September 2004
Abstract
Myelodysplastic syndromes (MDS) are clonal stem cell disorders, characterized by ineffective and dysplastic hematopoiesis. MDS
patients have a defective immune response manifested by increased susceptibility to bacterial infections, autoimmune phenomena, and high
incidence of lymphoid malignancies. Presently, we investigated the phenotype and function of monocyte-derived dendritic cells (MoDC) in
23 MDS patients and 15 controls at different stages of differentiation using the maturation stimuli tumor necrosis factor-alpha (TNF-a) and
LPS. Monocytes from MDS patients showed low potential to differentiate into dendritic cells (DC), as determined by low cell yield and
CD1a expression. MDS-MoDCs exhibited low expression of mannose receptor and reduced endocytic capacity. MDS-MoDCs showed a
diminished response to TNF-a with low CD83, CD80, and CD54 expression and allostimulatory capacity. In patients with 5q syndrome,
monocytes and MoDCs were positive for the 5q deletion, suggesting their origin from the malignant clone. Our data indicate that MoDCs in
MDS display quantitative and functional abnormalities that may contribute to the defective immune response of these patients.
D 2004 Elsevier Inc. All rights reserved.
Keywords: Myelodysplastic syndromes (MDS); Dendritic cells (DC); Maturation; Tumor necrosis factor-alpha (TNF-a)
Introduction
Myelodysplastic syndromes (MDS) are clonal disorders
of pluripotent hematopoietic stem cells occurring predom-
inantly in the elderly and characterized by ineffective hema-
topoiesis leading to peripheral blood cytopenias. There exist
clinical and laboratory data suggesting various defects of the
immune response in MDS such as increased susceptibility to
bacterial infections that are mainly due to the reduced
number and function of neutrophils [1], autoimmune
phenomena [2], and high incidence of lymphoid malignan-
cies [1–3]. In addition, progression of MDS to acute
myeloid leukemia and the increased risk of developing
1521-6616/$ - see front matter D 2004 Elsevier Inc. All rights reserved.
doi:10.1016/j.clim.2004.08.007
* Corresponding author. Hematology Division, Department of Internal
Medicine, Medical School and University Hospital, University of Patras,
Patras GR-26500, Greece. Fax: +30 2610 993950.
E-mail address: [email protected] (I. Micheva).
malignant tumors in MDS patients have been correlated to
impaired immune surveillance [2]. The reasons for the
immune disturbances observed in MDS patients remain
unclear; they may be due to primary defects of lymphoid
cells, of antigen (Ag) presenting cells (APC), or both.
Dendritic cells (DC) are the most potent APC, intimately
involved in the initiation and regulation of antigen-specific
immune responses [4]. DCs reside in a resting or immature
state in nonlymphoid tissues, where they efficiently capture
and process antigens. Upon activation, they initiate a dif-
ferentiation process that results in decreased Ag-processing
capacity, enhanced expression of MHC and costimulatory
molecules, and migration into secondary lymphoid organs,
where they trigger naive T-cells. This in vivo maturation
process is efficiently regulated and controlled by a complex
array of signals present in the DC microenvironment.
Recently, it has been shown that immature blood-derived
DCs in MDS originate from the malignant clone and exhibit
13 (2004) 310–317
I. Micheva et al. / Clinical Immunology 113 (2004) 310–317 311
phenotypic and functional deficiencies, and it was suggested
that DC dysfunction may account for the defective immune
response noted in MDS patients [5].
Circulating monocytes are considered a potential DC
precursor population, because they can differentiate into
DCs in vivo, providing a boost to the APC population in
sites of significant infection or inflammation [6]. In vitro,
DCs can be generated from peripheral blood monocytes
cultured with GM-CSF and IL-4 [7,8]. The monocyte-
derived DCs (MoDC) can be induced to mature by
immediate exposure to danger mediators such as bacterial
lipopolysaccharides (LPS) or proinflammatory cytokines,
mainly tumor necrosis factor-alpha (TNF-a) [9].
Presently, we studied the potential of peripheral blood
monocytes derived from the peripheral blood of patients
with MDS to differentiate into DCs. We further investigated
the phenotype and function of MoDCs at different stages of
maturation using the maturation stimuli TNF-a and LPS.
Materials and methods
Patients
Twenty-three patients with MDS and fifteen healthy
adults as controls were studied. Patients were diagnosed at
Patras University Hospital. Samples of heparinized blood
(20 ml) were drawn at the time of diagnosis and before the
administration of any treatment and from controls only
once. Informed consent was obtained from both patients and
controls. Patient data are presented in Table 1.
Table 1
Clinical characteristics of the MDS patients
MDS case FAB
category
Age
(years)
Sex
1 RA 67 M
2 RA 80 F
3 RA 60 F
4 RA 65 M
5 RA 72 M
6 RA 68 M
7 RA 62 M
8 RA 71 M
9 RARS 63 M
10 RARS 94 M
11 RARS 76 M
12 RARS 67 M
13 RARS 79 M
14 RAEB 69 F
15 RAEB 82 M
16 RAEB 58 M
17 RAEB 85 F
18 RAEB 69 F
19 RAEB 52 M
20 RAEB 69 F
21 CMML 80 M
22 CMML 61 M
23 CMML 69 M
Cells and culture conditions
Peripheral blood mononuclear cells (PBMC) were iso-
lated from venous blood by density gradient centrifugation
over Ficoll-Hypaque (Biochrom AG, Germany). CD3+ T-
cells were separated from PBMC using CD3 antibody-
coated immunomagnetic beads (Miltenyi Biotec, Glodbach,
Germany). CD3 T-cells were frozen in fetal bovine serum
(FBS) (Biochrom) with 10% dimethyl sulphoxide (DMSO)
(Sigma Chemical Co., St. Louis, MO) until further use.
PBMC were cultured at a concentration of 106 cells/ml in
culture medium (CM) composed of RPMI-1640, 10% FBS,
200 mmol/l l-glutamine, 50 Ag/ml streptomycin, and 50 U/
ml penicillin (all from Biochrom) for 2 h at 378C in a
humidified atmosphere of 5% CO2 in 25 cm2 tissue culture
flasks. The nonadherent cells were removed, the flasks were
washed, and the adherent cells were cultured in CM,
containing 100 ng/ml GM-CSF and 10 ng/ml IL-4
(Biosource, Nivelles, Belgium), for 5 days to obtain
immature DCs. MoDC were further cultured for 2 additional
days in plain CM or in the presence of 10 ng/ml TNF-a
(Biosource) or 0.1 Ag/ml lipopolysaccharide (LPS) (Escher-
ichia coli, serotype 055:B6) (Sigma). On day 5, cells were
counted using a hemocytometer. The percentage cell yield
was calculated as cell number obtained in culture over the
total cell number initially put into culture �100.
Flow cytometric analysis and sorting
Cells from the culture were washed, resuspended in FBS,
left for 1 h at 48C and then incubated with monoclonal
WBC
(� 109/l)
Mo
(%)/PBMC
Cytogenetics
9.2 4 46,XY,del(20q)
3.8 6 46,XX
6.3 6 46,XX
6.7 0.8 46,XY
2.8 0.7 47,XY,+8
5.6 4 46,XY
3.4 3.6 46,XY
3.78 7 46,XY
4.26 3.3 46,XY,del(5q)
8.1 3 46,XY
6.26 3 46,XY
4.8 3.6 46,XY
8.3 8 46,XY
3 4 46,XX
2.4 13 46,XY
1.7 0.5 46,XY
3.87 3 47,XX,+8,del5(q)
2.7 3.7 47,XX,+8
2.9 4 46,XY
5.2 10 46,XX,del(5q)
8.7 17 46,XY
12.5 28 46,XY
24.6 24 46,XY
Fig. 1. Mean DC yield after 5 days of culture in the presence of GM-CSF/
IL-4 for controls and MDS patients with RA, RARS, RAEB, and CMML.
I. Micheva et al. / Clinical Immunology 113 (2004) 310–317312
antibodies (mAbs) for 30 min at 48C. The following mAbs
were used: CD1a-PE, CD80-FITC, CD83-FITC, CD54-PE,
mannose receptor (MR)-PE (PharMingen, BD, Erembode-
gem, Belgium), HLA-DR-PE, CD11c-PE (BD), CD3-FITC
and PE, CD14-FITC (Immunotech, Villepinte, France),
TNFR1 (CD120a)-PE (Caltag Laboratories, Burlingame,
CA), and appropriate isotype-matched negative controls.
Nonviable cells were excluded from the analysis by gating
based on propidium iodide (PI) (PharMingen, BD). Samples
were analyzed on EPICS-XL (Beckman Coulter) flow
cytometer. Phosphate-buffered saline (PBS), supplemented
with 2% FBS was used as a staining buffer (SB) in the flow
cytometric assay. Before fluorescence in situ hybridization
(FISH), CD1a+/CD14� MoDCs were isolated with fluo-
rescence-activated cell sorting (FACS) (FACSVantage, BD)
and then used for cytospin preparation.
Mannose receptor-mediated endocytosis
DCs were incubated in CM with dextran-FITC (MW
40000, Sigma) at a concentration of 1 mg/ml for 30 min at
378C and also at 48C to determine the background uptake.
DCs were washed four times with ice-cold SB in a refrigera-
ted centrifuge and analyzed immediately by flow cytometry.
Dextran uptake was evaluated by the mean fluorescence
intensity (MFI) of the FITC channel and calculated in
arbitrary units (AU) as (MFI378C � MFI48C)/MFI48C.
Mixed lymphocyte reaction (MLR)
MoDCs were treated with mitomycin C (Sigma) (50 mg/
ml) as previously described [10]. DCs were then cocultured
with allogeneic normal CD3+ T-cells in varying ratios (1:5,
1:10, 1:20, and 1:100). Cultures were maintained in a
humidified atmosphere at 378C and 5% CO2 for 5 days.
Bromodeoxyuridin (BrdU), 10 AM, was added for the last
16 h. T-cell proliferation was assessed by the BrdU
incorporation using three-color staining flow cytometry
assay with anti-BrdU-FITC, CD3-PE monoclonal antibod-
ies, and 7-amino-actinomycin-D (7AAD) as instructed by
the manufacturers (PharMingen, BD).
FISH analysis
FISH was performed on CD1a+ MoDCs in two patients
with 5q abnormality. Cells were fixed in methanol–acetic
acid (3:1) and stored frozen at �208C until further use. FISH
analysis was performed using the LS1 EGR1/D5S721:
D5S23 dual-color DNA probe (Vysis Inc., Downers Grove,
USA), which hybridizes to regions 5q31 (SpectrumOrange
LS1 EGR1) and 5p15.2 (SpectrumGreen LS1 D5S72, D5
S23). Cells were denatured, dehydrated in a graded (70%,
85%, 100%) series of ethanol, air-dried, and hybridized
with the probe for a period of 16–18 h. Slides were washed
with x3 in 50% formamide/2� SSC, x1 in 2� SSC, and x1
in 2� SSC/0.1% NP-40. Each wash was at 468C for 10 min.
Slides were then counterstained with 125ng/ml DAPI
(4V,6-diamidine-2V-phenylindole; Boehringer Mannheim,
Germany) and viewed on a Zeiss Axioskop fluorescent
microscope. Image enhancement was performed using the
Isis 3 software (Metasystems GmbH, Germany).
Statistical analysis
Kolmogorov-Smirnov test was initially applied to deter-
mine whether the distribution of the values could be
considered normal. The independent data sets were com-
pared using independent two-tailed t tests. The paired
observations were analyzed using paired t tests. P b 0.05
was considered significant. The Pearson correlation test was
used to assess linear relationships between samples.
Results
Impaired differentiation of MDS blood monocytes into DC
At the end of the culture period (5 days) in the presence
of GM-CSF and IL-4, 8.2% F 3.8% of the PBMC from the
controls and 4.9% F 2.9% of the PBMC from the MDS
patients with RA, RARS, and RAEB differentiated into
MoDCs (P = 0.01). In the three cases with CMML, the cell
yield was higher, compared to the controls and the other
MDS types (Fig. 1). In all MDS cases, there was no
correlation between the percentage of monocytes in the
PBMC fraction at the beginning of the culture (range 0.5–
13%) and the DC yield (r = 0.388), whereas a positive
correlation was calculated for normal donors (r = 0.56).
Phenotypic characteristics of MoDC at different stages of
maturation
Immunophenotypic studies were performed on the
obtained immature MoDCs and on MoDCs stimulated with
TNF-a or LPS. Large cells with increased forward and side
scatter comprised the MoDC population. The percentage of
the viable cells, represented by the PI-negative DC
population, was higher than 92%; their myeloid origin
was confirmed by the expression of myeloid DC marker
CD11c. In MDS patients, the expression of CD1a and CD80
was
significan
tlylower
com
expressio
nof
otherDC-as
(CD83,HLA-D
R,andCD54
patien
tsandcontro
ls(Fig.2,
Theim
matu
reMDS-M
oD
nifican
tlylower
levels
than
M
2.24F
0.5
vs.MFI5.22F
2
Fig.2.P
CSF/IL
-4
gensbef
henotypeofDCsgenerated
andstim
ulated
with
TNF-a
ore
andafter
stimulatio
nin
M
pared
tothe
contro
ls.The
sociated
surfa
ce
molecules
)was
similar
betw
eenMDS
Table
2).
Csexpressed
TNFR1at
sig-
oDCsfro
mthecontro
ls(M
FI
.47,P=0.02)(Fig.3).
from
PBMCsin
thepresen
ceofGM-
orLPS.Expressio
nofDCsurface
anti-
DSpatien
tsandcontro
ls(*Pb0.05).
Table 2
Surface antigen expression (mean MFI F SD) on DCs from MDS patients (MDS) and from healthy subjects (C)
Immature DCa TNF-ab LPSc C—P values MDS—P values
C MDS P C MDS P C MDS P I/T I/L T/L I/T I/L T/L
CDla 11.1 F 6.1 6.8 F 4.7 0.034 4.3 F 2.1 8.2 F 5 0.07 3.7 F 1.8 3 F 2.6 0.552 0.02 0.07 0.577 0.976 0.011 0.01
CD83 0.4 F 0.3 0.47 F 0.3 0.793 2.2 F 1.1 0.9 F 0.6 b0.00l 3.5 F 1.9 2.3 F 1.6 0.155 0.001 0.003 0.087 0.013 0.004 0.002
CD80 2.1 F 0.4 0.7 F 0.5 b0.00l 3.5 F 1.5 1.2 F 1.2 b0.00l 6.2 F 3.9 6.2 F 3.1 0.992 0.033 0.025 0.085 0.099 0.002 0.001
CD54 54.1 F 15.7 62.2 F 27.9 0.328 103.1 F 21 66.4 F 25.1 0.005 88.3 F 9 110.7 F 29.9 0.065 0.001 b0.001 0.091 0.218 0.012 0.006
HLA-DR 54.9 F l8.8 51.1 F 20.4 0.619 117.2 F 38.9 91.8 F 31.6 0.105 180.6 F 32.6 166.7 F 34.5 0.427 0.001 b0.00l 0.004 b0.00l b0.00l b0.00l
MR 24.9 F 7.2 17.3 F 12.8 0.001 11 F 2.1 12.5 F 8.6 0.639 6.6 F 1.5 11.2 F 2.5 0.001 b0.00l 0.006 0.002 0.08 0.08 0.814
Differences between healthy volunteers and patients are analyzed using two-tailed t test; differences between immature and mature DCs and between maturation stimuli are calculated using t test for paired
samples; P values are shown for each analysis.a Immature DC (I).b DC stimulated with TNF-a (T).c DC stimulated with LPS (L).
I.Mich
evaet
al./Clin
icalIm
munology113(2004)310–317
313
Fig. 3. Comparison of the expression of TNFR1 (CD120a) on MoDCs
obtained in GM-CSF/IL-4: (a) results of the flow cytometry analysis of a
representative control and MDS patient; (b) comparison of the mean values
of expression.
Fig. 4. Dextran-FITC endocytosis (a) and MR expression (b) of immature,
TNF-a-, or LPS-matured MoDCs from patients with MDS and controls (*P
b 0.05).
Fig. 5. Allogeneic stimulatory activity of MoDCs. Mitomycin C-treated
DCs were cultured with allogeneic normal CD3 cells in different ratio (a).
T-cell proliferation was assessed by the BrdU incorporation. The mean
percentage of BrdU-positive proliferating lymphocytes for ratio 1:10
stimulator to responder cells before and after stimulation with TNF-a or
LPS in MDS patients and controls is represented on the graph (b) (*P b
0.05).
I. Micheva et al. / Clinical Immunology 113 (2004) 310–317314
In controls, culture of immature MoDCs with LPS and
TNF-a resulted in a significant up-regulation of DC surface
marker CD83, costimulatory molecule CD80, adhesion
molecule CD54, and HLA-DR. In MDS patients LPS was
an efficient stimulator of immature MoDCs, inducing
significant up-regulation of the intensity of expression of
CD83, CD80, HLA-DR, and CD54 and down-regulation of
the expression of CD1a. In contrast, TNF-a failed to induce
maturation of MDS-MoDCs, because alterations of the
expression of CD83, CD80, and CD54 markers were
negligible and remained significantly lower than in controls
(Fig. 2, Table 2).
Low endocytic capacity of MDS-MoDC with low expression
of mannose receptor
The capacity of MoDCs to uptake soluble antigens was
assessed by their ability to endocytose dextran-FITC. The
endocytic capacity of immature MDS-MoDCs was signifi-
cantly reduced in comparison to control-MoDC (2.0 F 1.1
AU vs. 3.42 F 0.6 AU, P = 0.03). When control immature
MoDCs were induced to maturation with either TNF-a or
LPS, a significant down-regulation of the dextran-FITC
endocytosis was observed. MDS-MoDCs, stimulated by
both maturation factors, exhibited no further decrease of
their endocytic activity (Fig. 4a).
The low dextran endocytosis of immature MDS-MoDCs
was accompanied by significantly lower, compared to
controls, expression of MR (P = 0.02) that was slightly
down-regulated upon maturation with both LPS and TNF-a
(Fig. 4b).
Allogeneic stimulatory capacity of MoDC at different stages
of maturation
We investigated the ability of immature as well as LPS-
or TNF-a-stimulated MoDCs to induce proliferation of T-
cells in an allogeneic MLR. The optimal DC–T-cell ratio
was 1:10 (Fig. 5a). Upon TNF-a stimulation, MDS-MoDCs
Fig. 6. FISH analysis of sorted CD1a+ MoDCs from a patient with 5q
syndrome (a) and a healthy subject (b). Normal nuclei appear with four
distinct signals, two green (5p) and two orange (5q), whereas the del
(5)(q13q33) aberration is indicated by nuclei containing two green and one
orange signal. (For interpretation of the references to color in this figure
legend, the reader is referred to the Web version of this article.)
I. Micheva et al. / Clinical Immunology 113 (2004) 310–317 315
failed to up-regulate the proliferative response in T-cells.
Immature MoDCs and MoDCs stimulated with LPS from
both MDS patients and controls did not differ in their ability
to induce proliferation of allogeneic T-cells (Fig. 5b).
Derivation of DC from the dysplastic clone in MDS
To determine the clonal origin of MoDCs in MDS, FISH
analysis was performed on sorted CD1a+ MoDCs from two
patients with 5q syndrome. In both cases, almost all CD1a+
DCs (94% and 95%, respectively) appeared to be derived
from the 5q deletion clone. Cell cytospins from controls
consistently had less than 6% of nuclei with 2 G + 1 O
signal pattern (Fig. 6).
Discussion
MDS are characterized by ineffective hematopoiesis with
impaired proliferation and maturation of one or more cell
lineages in the bone marrow, resulting in PB cytopenia.
Various immune disturbances in MDS such as increased
susceptibility to bacterial infections, autoimmune phenom-
ena, and high incidence of lymphoid malignancies [1–3]
reveal an underlying defect of the immune response in MDS
patients; the reasons for which still remain unclear.
A previous report [5] has shown that, in eight patients
with MDS, the immature MoDCs are phenotypically
defective with decreased expression of CD1a, CD54,
CD80, and class II molecules and exhibit low endocytic
as well as allostimulatory activity. In cases with trisomy 8
and monosomy 7 MDS, MoDCs were positive for the
cytogenetic aberration.
In the present study, we generated DCs from peripheral
blood monocytes in 23 patients with MDS and investigated
their phenotype and function in different stages of matura-
tion. The induction of DC with GM-CSF and IL-4 was
possible in all patients. However, we found that, in RA,
RARS, and RAEB, the yield of MDS-MoDCs was
significantly lower than in controls, whereas no difference
was found in CMML, in agreement to a previous study [11].
The low DC yield together with the fact that MDS
monocytes were positive for the 5q deletion suggests that
monocytes from patients with MDS originate from the
malignant clone and have low potential to differentiate into
DCs.
The immature MDS-MoDCs, generated in the presence
of GM-CSF and IL-4, had a reduced expression of CD1a
and CD80 surface antigens, but no difference was found
concerning the other DC-associated markers. Respectively,
the immature MoDCs in MDS did not differ from controls
in their ability to induce proliferation of allogeneic T-cells.
CD1a is a surface receptor involved in the antigen
uptake, and CD80 is a costimulatory molecule implicated in
the induction of antitumor immunity [12]. The reduced
expression of CD80 may be associated with the increased
incidence of other malignancies, and particularly lymphoid
neoplasms, observed in MDS patients and the escape of the
malignant clone from immune control with progression
towards acute leukemia.
The ability of DCs to take up and process antigens is
highly dependent on the stage of DC differentiation. The
high endocytic capacity is a specific property of cultured
immature DCs and is down-regulated upon maturation [7].
We studied the capacity of MDS-MoDCs to take up soluble
antigens via MR, a major antigen uptake receptor on
immature MoDCs. It has been previously reported that
mannosylated antigen is efficiently internalized by MR on
MoDCs, processed, and presented to T lymphocytes [13] We
found a reduction of the endocytic ability of immature DCs
with an insufficient down-regulation of endocytosis after
TNF-a and LPS induced maturation. We also observed a
significant reduction of the MR expression on DCs derived
from MDS patients, suggesting that a quantitative defect of
MR probably accounts for the impaired endocytosis.
The low endocytic ability may contribute to an inefficient
response to danger signals, contributing thus to the
infectious complications in MDS. Several studies have
shown that excessive apoptosis is a characteristic feature of
MDS [14,15]. DCs are involved in the apoptotic cell
I. Micheva et al. / Clinical Immunology 113 (2004) 310–317316
clearance, although not as efficiently as macrophages.
Physiologically, the apoptotic cell engulfment from DCs
prevents the onset of autoimmune reactions [16]. If
excessive apoptosis coincides with poor clearance, the
persistence of apoptotic bodies may promote an inflamma-
tory response or present a source of antigens [17]. In this
regard, the decreased endocytic capacity of immature DCs
may be implicated in the pathogenesis of autoimmune
disorders commonly seen in MDS.
Another interesting observation in the present study was
that MDS-MoDCs respond differently to the stimulating
agents LPS and TNF-a. LPS, but not TNF-a, induced
complete phenotypic and functional maturation of the MDS-
MoDCs. The bacterial cell wall constituent of LPS functions
as a physiological stimulus for DC maturation. In vitro LPS
stimulates MoDCs to produce IL-6, IL-8, IL-12, and TNF-
a, to up-regulate costimulatory molecules, and to accumu-
late rapidly stable peptide-loaded MHC class II molecules
[18]. TNF-a influences the DC growth and differentiation
characterized mainly by dendritic morphology, expression
of high levels of MHC, adhesion and costimulatory
molecules (HLA-DR, CD40, CD80, CD86), and low or
absent phagocytic but strong antigen-presenting capacity
[19]. Furthermore, it has also been reported that the
mediator of TNF-a induced signaling during DC maturation
is TNFR1 [20].
In the present study TNF-a failed to induce maturation of
MDS-DCs as shown by low expression of surface markers
(CD80, CD83, and CD54) that are presumably important for
DC–T-cell interaction. Besides the phenotypical defect,
TNF-a-stimulated DCs were poor inducers of T-cell
proliferation in MLR.
The maturation failure to TNF-a could be assigned to the
reduced expression of TNFR1 reported in our study. This
finding is of interest, since there is evidence for a role of
TNF-a in MDS pathogenesis. Several studies indicate that
TNF-a is elevated in the bone marrow [21,22] and
peripheral blood [23–25] of MDS patients. It is conceivable
that the chronic exposure to TNF-a could result in down-
regulation of TNFR1.
Alternatively, the differential effect of TNF-a and LPS
on the maturation of DCs could be related to defects of the
intracellular pathways triggered by TNF-a. The activation
of NF-nB family members is a critical control pathway for
differentiation of monocytes to DCs and for maturation of
DCs from antigen-processing to antigen-presenting cells
[26]. NF-nB transcription factor regulates a large number of
genes involved in immune responses, such as the proin-
flammatory cytokines (IL-1, IL-6, TNF-a) and cell surface
molecules including CD80 [27]. In this context, it can be
hypothesized that the difference in MDS-MoDCs matura-
tion by TNF-a and LPS reflects an underlying defect in the
capacity of TNF-a to activate NF-nB. It has been reported
that the capacity of DCs to activate T-cells following
CD40L treatment was enhanced compared with TNF-a
treatment, and this effect was NF-nB-dependent [28].
In conclusion, MDS-MoDCs belong to the abnormal
MDS clone and exhibit quantitative and functional abnor-
malities. Although functionally active when stimulated with
LPS, the MDS-MoDCs were numerically deficient and
showed low endocytic ability and impaired maturation after
TNF-a stimulation. This constellation of DC defects may
contribute to the defective immune response against
pathogens, escape and expansion of the malignant clone,
as well as autoimmune phenomena, observed in MDS
patients.
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