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Improving the differential diagnosis between myelodysplastic syndromes and reactive peripheral cytopenias by multiparametric flow cytometry: the role of B-cell precursors
Diagnostic Pathology volume 10, Article number: 44 (2015)
Immunophenotyping is a valuable ancillary technique for the differential diagnosis between myelodysplastic syndromes (MDS) with low bone marrow (BM) blast counts and a normal karyotype, and reactive peripheral (PB) cytopenias. Our aim was to search for the most important variables for this purpose. We also analyzed the age variation of BM B-cell precursors (BCP) and its differences in reactive and clonal cytopenias.
Immunophenotypic analyzes were performed in BM of 54 patients with MDS (76% with BM blasts <5%) and 35 cases of reactive cytopenias. Healthy allogeneic BM transplantation donors (n = 41) were used as controls. We used a four-color panel of antibodies analyzing 9 granulocytic, 8 monocytic and 6 CD34+ cell features.
Asynchronous shift to the left in maturing granulocytes and increase in CD16+ monocytes were also found in reactive PB cytopenias, but the most important aberrancies in MDS were seen in myeloid CD34+ cells. Decrease in BCP, that is a hallmark of MDS, could also be found in reactive cytopenias, especially in patients >55 years. % BM BCP could be calculated by the formula: (−7.97 × log age) + (4.24 × log % CD34 + cells) – (0.22 x nr. alterations CD34 + cells) + 0.577. Corrected R2 = 0.467.
Analysis of myelomonocytic precursors and CD34+ cells was satisfactory for the differential diagnosis between reactive PB cytopenias and MDS. The most specific alterations were found in CD34+ cells. Comparison of the values obtained with those of normal age-matched controls is recommended.
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In the last years, numerous studies have confirmed the utility of multiparametric flow cytometry (FCM) in the diagnosis of myelodysplastic syndromes, especially in cases with a normal karyotype, and its differential diagnosis with peripheral cytopenias of non-clonal origin [1-10]. FCM of BM hemopoietic precursors has been focused mainly on myelomonocytic precursors and CD34+ progenitors. There is no single specific abnormality, but the presence of three or more aberrancies may strongly support the diagnosis of MDS [1,2].
Several kinds of phenotypic abnormalities have been described in MDS such as a low SSC in granulocytic precursors, loss of antigen expression, asynchronous maturation or maturation block, aberrant cross-lineage co-expressions, quantitative and qualitative abnormalities of CD34+ cells, along with the decrease of precursor B cells (BCP) [9,11-21]. Many phenotypic abnormalities found in CD34+ cells have been associated with disease progression and are able to predict a shorter survival of the patients [5,8,10,15,17,19,20,22-31].
According to the European Leukemia Net Working Group (ELN) standardization [3,6,31], BM immunophenotyping in MDS should at least focus on the maturation of myelo-monocytic precursors as well as the enumeration of hemopoietic progenitors and BCP. So, a minimal panel should be designed to detect all these abnormalities [3,5,8,22,31]. Furthermore, comparison with the normal pattern of antigen expression of each lineage and maturation step should be performed. Besides, several scores based on phenotypic findings have been described to support the differential diagnosis between MDS and reactive PB cytopenias, but there is no general consensus indicating the best one for application in daily routine [5,8,10,15,17,23,25-31].
In our previous studies [10,19,23], we have analyzed the utility of a four-color panel that was able to detect several phenotypic abnormalities in the myelomonocytic series and CD34+ cells. We have also found that maturation abnormalities of myelomonocytic precursors are similarly present in all WHO types of MDS, while those detected in CD34+ cells are the most important to predict a shorter survival of the patients [19,20]. Recently, comparing the prognostic value of IPSS, IPSS-R and WPSS with those obtained by flow cytometry, we found that CD34+/CD13+ cells and total number of phenotypic alterations found in the myelomonocytic series and CD34+ cells were additional independent prognostic factors to the clinical scores .
Here, our aim was to examine which abnormalities detected by our panel were more important for the differential diagnosis between reactive PB cytopenias and cases of MDS with a normal karyotype. As the number of BM B-cell precursors is age-dependent, we also examined the impact of this variation in the utility of this feature in the differential diagnosis.
Patients and samples
Since December of 2009, immunophenotyping was included in the diagnostic work-up of peripheral cytopenias in our Institution together with PB counts, BM cytology and karyotyping. The WHO criteria were used for the diagnosis of MDS and exclusion of deficiency anemias, viral infections, auto-imune diseases and renal or hepatic insufficiency was made [1,2]. During the period of the study (December 2009 – February 2013), we could confirm the diagnosis of MDS in 56 cases while in 35 cases the final diagnosis of reactive cytopenias was made (Table 1). Twenty five patients were excluded because of lack of complete clinical data or uncertain diagnosis.
The classification of the MDS cases was made according to the WHO criteria and risk category according to IPSS, IPSS-R  and WPSS (using hemoglobin values instead of “transfusion dependency”)  was assessed.
Cytogenetic analysis of BM was performed after 24 hours of culture according to standard methods. In each case, at least 20 mitoses were analyzed and the karyotypes were reported according to the International System for Human Cytogenetic Nomenclature .
Normal BM samples were obtained from 41 healthy donors for allogeneic bone marrow transplantation (age: 15–69 years) in order to standardize a normal immunophenotypic profile for our laboratory. All samples were collected during the period between July 2009 and January 2013.
All BM samples were obtained after informed consent was given by each person, according to the recommendations of the local Ethics Committee (proc. Nr. 0652.0.146.000-08).
Flow cytometry analyses
Immunophenotyping was performed as previously described [10,19]. Briefly, the EDTA-anticoagulated BM sample (5-7 × 106 cells in 100 μl per test) was processed using a standardized direct lyse-and-wash technique within 24 hours after bone marrow aspiration . Quality control, calibration and compensation with FACS Comp were performed daily in our equipment.
Antigenic expression was studied using four-color combinations of monoclonal antibodies (MoAbs) conjugated with fluorescein isothiocyanate (FITC), phycoerythrin (PE), peridin clorophyll protein (PerCP) and allophyicocyanin (APC) fluorocromes. The following combinations were used to study the myelomonocytic maturation and progenitor cell populations: HLA-DR/CD14/CD45/CD33; CD16/CD11b/CD45/CD13; CD13/CD34/CD45/CD117; CD10/CD19/CD45/CD34; CD7/CD56/CD45/CD34. The specificity and source of each reagent have already been described in detail . Immediately after staining, samples were acquired in a FACS Calibur flow cytometer (Becton Dickinson – BD Biosciences) using the CellQuest software (BD Biosciences). Instrument quality control, calibration using FacsComp™ (BD) software and spectral compensation were performed daily. Information about at least 100,000 nucleated BM cells was acquired for each sample. Data analysis was made using Infinicyt software (Cytognos). The strategies of analysis were standardized as previously described [10,19,23]. These variables also were assessed in normal BM.
The analysis of the myelomonocytic series was made as previously described  according to ELN standardization [3,27,31]. Briefly, maturation pattern of neutrophils was analyzed by their expression of CD13, CD16, CD11b, CD33 and HLA-DR. The side-scatter (SSC) of the granulocytic population and the antigen expressions were considered abnormal if the values of the mean fluorescence intensity (MFI) were above or below the benchmark values obtained for the normal cases (Table 2). Monocytes were analyzed by their expression of HLA-DR, CD64 and CD14. The combination CD16/CD11b/CD45/CD13 was used to quantify the CD16+ monocytes. The aberrant expression of CD34, CD7 and CD19 was investigated in each population considering abnormal when at least 10% of the cells expressed these antigens. For expression of CD56 in the myelomonocytic cell line, only values of >20% for granulocytes and >50% for monocytes were considered abnormal.
CD34+ cells were separated in the SSC/CD34 dot plot [10,19] (Figure 1) and their co-expression of CD19, CD10, CD13, CD117, CD7 and CD56 was examined. The B-cell precursors (CD34+/CD19+/CD10+) were measured as percentage of the total nucleated cells.
All immunophenotypic features were compared with the values found in normal BM. We computed the total number of granulocytic and monocytic abnormalities, as well as those of CD34+ cells. We also computed the sum of all abnormalities found.
The mean values and standard deviation were obtained for all variables analyzed. The difference between groups was assessed by analysis of variance. The normal distribution of the features of normal hemopoiesis was examined by the Kolmogorov-Smirnov test, and those with a non-normal distribution were submitted to a log transformation. The relation of B-cell precursors with age and among the groups studied was examined using the Spearman rank order correlation and multiple regressions. Values were considered significant when p < 0.05. The Winstat and SPSS.15 softwares were used for the calculations.
Concerning patients with MDS, the majority were RCMD (Table 1). In 5 cases no mitoses were available for karyotyping. As some of the patients’ groups in IPSS-R and WPSS classification were rather small, we grouped the cases with <5% BM blast (low risk) and MDS with > 5% BM blast (high risk) for analysis. A major part of the patients were low and intermediate risk in all clinical scores analyzed and had BM blasts <5%.
The cases with non-clonal cytopenias included deficiency anemias (n = 11), drug-induced cytopenias (n = 6), aplastic anemia (n = 3), idiopathic thrombocytopenic purpura (n = 4), auto-immune diseases (n = 4), thyroid dysfunction (n = 3), and infection-associated leucopenia (n = 4). There were 15 men and 20 women with a median age of 60 years (14–86).
The normal values were established by the analysis of 41 normal donors of allogeneic bone marrow transplantation with a median age 32 years (15–69); 25 males and 16 females. All features examined except for MFI for SSC in the granulocytic precursors and total B-cell precursors presented a normal distribution. So we used the mean values obtained ± 2 standard deviations except for MFI SSC of myelomonocytic cell lines and percentage of total B-cell precursors. For these two features we used the 5% and 95% percentiles, due to the large variation observed in the normal controls.
Flow cytometric data of non-clonal cytopenias are shown in Table 2. There was no abnormality concerning SSC of granulocytes and monocytes. Shift to the left, with asynchrony of antigen expression was found in 7 cases (Table 3). In two cases, abnormal maturation pattern in CD13 or CD16 was observed in maturing granulocytes. There was one case with an autoimmune disorder presenting expression of CD34 in maturing granulocytes without any other abnormality, and one with hepatitis C at diagnosis presenting expression of CD7 in maturing granulocytes. In 9 cases (26%), increased percentages of monocytes were found.
There was an increase of CD16+ monocytes in 8 cases of reactive cytopenias. A statistical difference was found among normal, reactive cytopenias and MDS. CD56 was expressed in monocytes in 2 cases, CD7 and CD19 were expressed in one case each (cases with deficiency anemia).
The percentage of total CD34+ cells and %CD34+/CD117+/CD13+ cells (myeloid blasts) were increased in only one case of deficiency anemia, associated with a shift to the left in the granulopoiesis. CD56 was expressed in 2 cases (0.06% and 0.09% of the cells). B-cell precursors were below the normal value in 14 cases (41%). All these alterations resulted in an increased number of total abnormalities.
Abnormalities observed in MDS
The abnormalities found in MDS are also shown in Tables 2 and 3. Most of the aberrancies studied were more common in MDS than in reactive cases. Concerning CD34+ cells, they were increased in 26% of the cases of MDS with BM blast count <5% in cytology and in 83% of the cases with RAEB. The same was true for the cells with the phenoptype CD34+/CD13+/CD117+ (Table 3). Abnormal co-expressions were rare in reactive cytopenias and common in MDS (Table 3).
Relation between B-cell precursors and age
Considering all the subjects studied, the median age was 55 years. Within the groups, normal subjects had a median age of 32 years (range: 15–69); reactive cytopenias: 60 years (range: 14–86) and MDS: 69 years (range: 15–84).
In the Spearman’s test, there was a negative correlation between age and BCP in all three groups: r = − 0.328; p 0.023 for healthy donors; r = − 0.321; p = 0.032 for reactive cytopenias (Figure 2A) and r = − 0.412; p = 0.002 for MDS cases (Figure 2B). These cells were absent in none of the normal donors, in 8/35 cases of reactive cytopenias and in 33/54 cases of MDS.
Among the subjects with age <55 years, mean B-cell precursors were 0.18%, 0.14% and 0.17% in normal controls, reactive cytopenias and MDS cases respectively, which was not significantly different. Among subjects >55 years old, mean values were 0.28%, 0.075% and 0.015% respectively. These values were significantly different (p < 0.005).
In the multiple regressions considering age, total % CD34+ cells, BCP and number of alterations in CD34+ cells, the relation could be described in non-clonal subjects (normals and reactive cytopenias) by the equation:
For the MDS cases the equation was:
Several immunophenotypic abnormalities have been described in MDS. According to the WHO 2008 recommendations , the finding of three or more abnormalities is considered highly suggestive of MDS. Thus, immunophenotyping has been considered a useful adjuvant method for the diagnosis of MDS in cases with low BM blast counts and a normal karyotype . This technique is also widely used for the diagnosis and assessment of minimal residual disease in several other hematological neoplasms [35,36].
Knowledge of normal antigen expression of the several hemopoietic cells and its changes during normal cell maturation is essential to assess abnormalities and to define leukemia-associated immunophenotypes (LAIPs) [3,8]. It is also advisable for each laboratory to establish their own reference normal values for each panel of monoclonal antibodies used. In healthy individuals, normal maturation of BM precursors is genetically tightly controlled, leading to predictable patterns of antigen expression at different stages of cell maturation. Neoplastic cells are characterized by a deviation of this pattern, as well as by the presence of aberrant cross-lineage antigen expressions [4,5,8,12,37].
In previous studies [10,12,19,23], we have shown that a rather small four-color panel of monoclonal antibodies analyzing the myelomonocytic lineage and the subsets of CD34+ cells was suitable to confirm the diagnosis of MDS and allowed us to detect independent prognostic features . Among the phenotypic abnormalities found, those concerning CD34+ cells were the most important to predict a shorter survival of the patients. At last we substituted the combination for analysis of dendritic cells and basophils for a combination (CD7/CD56/CD45/CD34) to assess the most frequent leukemia-associated phenotypes. Both minor populations are altered in MDS, but are less important for the differential diagnosis of clonal and non-clonal cytopenias.
In the present work, our aim was to examine which variables detected by our panel were more important to discriminate between reactive PB cytopenias and MDS, especially in those cases with few BM blasts and a normal karyotype. Concerning the variables analyzed, our reactive cases never presented a decreased SSC or a maturation block in the myeloid series. Shift to the left was seen in 7 cases and abnormal expression of CD13 was seen in 2 cases. This is in keeping with the fact that, although variation in antigen expression may occur in reactive cytopenias, the rupture of the normal pattern of maturation should never be seen, as this is indicative of a clonal disorder.
Concerning monocytes, increase in number and expression of CD16 and CD56 that are indicative of cell activation, were observed, although this was more frequent in MDS, as it also has been observed by others .
The main immunophenotypic features distinguishing low-risk MDS from reactive cytopenias were the increase of CD34+ cells, especially in the presence of normal blast counts in cytology, increase in CD34+/CD117+/CD13+ cells, decrease in B-cell precursors, and aberrant co-expressions in CD34+ cells (CD7 or CD56 or decrease in CD13). The presence of anomalous expression of CD7 in CD34+ cells was more frequent in high-risk MDS and might reflect progression to leukemia.
The total number of phenotypic abnormalities was also significantly higher in clonal disorders, confirming previous results of our group and others [12,19,24-28]. Overall, in patients with reactive cytopenias, if phenotypic abnormalities are found, a close follow-up of the patient should be made in order to detect a possible evolution to an overt MDS.
The decrease of B-cell precursors has been considered a hallmark of MDS [6,9,13,21,31], even in children. This variable has also been included in phenotypic scores for diagnosis of MDS, such as that proposed by Ogata and included in the guidelines of ELN . B-cell precursors may be assessed as CD34+ cells with a low SSC or by their phenotype, which is the way to obtain more reliable results. We also assessed these cells as their percentage among all cells examined and not as percentage of all CD34+ cells, as has been recommended by several authors [11,24,30,37]. In MDS it is expected that myeloid progenitors may be increased, provoking a false relative decrease of B-lymphoid precursors. So, the best way to evaluate their number would be to use their percentage among all cells.
On the other hand, it is well known that the number of BM B-cell precursors have a strong variation with age . This was also the case in the present study. We could show that in a multiple regression, their number was dependent of age and the total number of CD34+ cells. In MDS, also the total alterations observed in CD34+ progenitors entered the equation.
In subjects with age below 55 years the difference in number of BCP was not so pronounced, but in older patients, their number was below normal in reactive cytopenias and this was more pronounced in MDS. This is in keeping with an ageing process of the immune system, which is highly variable with age and amount of exposure to antigen stimulation. The pathophysiology of the decrease of B-cell precursors observed in MDS is not well understood. But, it has been described that these cells may also present abnormalities in antigen expression in MDS  that are more pronounced in cases with a higher number of BM blasts. This could be due to a more pronounced dysfunction of hemopoietic progenitors that loose their capacity to produce the B-cell line.
In conclusion, an antibody panel focused on the analysis of the myelomonocytic cell line and CD34+ cells was satisfactory for the differential diagnosis between reactive PB cytopenias and MDS with low BM blast counts and a normal karyotype. The most specific alterations were found in CD34+ cells. The number of BCP was more discriminative in older patients. For young patients it is necessary to compare their number with normal age-matched subjects.
European Leukemia Net Working Group
World Health Organization
International Prognostic Scoring System
Revised International Prognostic Scoring System
WHO classification-based Prognostic Scoring System
Peridin clorophyll protein
Median fluorescence intensity
Refractory cytopenia with multilineage dysplasia
Refractory anemia with excess blasts
Absolute neutrophil count
Swerdlow S, Camp E, Harris NL, Jaffe ES, Pileri SA, Stein H, et al. WHO classification of tumors of haematopoietic and lymphoid tissues. Lyon: IARC; 2008.
Valent P, Horny HP, Bennett JM, Fonatsch C, Germing U, Greenberg P, et al. Definitions and standards in the diagnosis and treatment of the myelodysplastic syndromes: Consensus statements and report from a working conference. Leuk Res. 2007;31:727–39.
van de Loosdrecht AA, Alhan C, Béné MC, Della Porta MG, Dräger AM, Feuillard J, et al. Standardization of flow cytometry in myelodysplastic syndromes: report from the first European LeukemiaNet working conference on flow cytometric in myelodysplastic syndromes. Haematologica. 2009;94:1124–34.
Stetler-Stevenson M, Yuan CM. Myelodysplastic syndromes: the role of flow cytometry in diagnosis and prognosis. Int J Lab Hematol. 2009;31:479–83.
Ossenkoppele GJ, van de Loosdrecht AA, Schuurhuis GJ. Review of the relevance of aberrant antigen expression by flow cytometry in myeloid neoplasms. Br J Haematol. 2011;153:421–36.
Della Porta MG, Picone C, Pascutto C, Malcovati L, Tamura H, Handa H, et al. Multicenter validation of a reproducible flow cytometric score for the diagnosis of low-grade myelodysplastic syndromes: results of a European LeukemiaNET study. Haematologica. 2012;97:1209–17.
Loken MR, van de Loosdrecht A, Ogata K, Orfao A, Wells DA. Flow cytometry in myelodysplasic syndromes: report from a consensus working conference. Leuk Res. 2008;32:5–17.
van de Loosdrecht AA, Westers TM, Westra AH, Drager AM, van der Velden VH, Ossenkoppele GJ. Identification of distinct prognostic subgroups in low- and intermediate-1-risk myelodysplastic syndromes by flow cytometry. Blood. 2008;111:1067–77.
Sandes AF, Kerbauy DM, Matarraz S, Chauffaille ML, Lopez A, Orfao A, et al. Combined flow cytometric assessment of CD45, HLA-DR, CD34, and CD117 expression is a useful approach for reliable quantification of blast cells in myelodysplastic syndromes. Cytometry B Clin Cytom. 2013;84:157–66.
Reis SC, Traina F, Saad STO, Lorand-Metze I. Variation of bone marrow CD34+ cell subsets in myelodysplastic syndromes according to WHO types. Neoplasma. 2009;56:435–40.
Satoh C, Dan K, Yamashita T, Jo R, Tamura H, Ogata K. Flow cytometric parameters with little interexaminer variability for diagnosing low-grade myelodysplastic syndromes. Leuk Res. 2008;32:699–707.
Lorand-Metze I, Ribeiro E, Lima CSP, Batista LS, Metze K. Detection of hematopoietic maturation abnormalities by flow cytometry in myelodysplastic syndromes and its utility for the differential diagnosis with non-clonal disorders. Leuk Res. 2007;31:147–55.
Aalbers AM, van den Heuvel-Eibrink MM, Baumann I, Dworzak M, Hasle H, Locatelli F, et al. Bone marrow immunophenotyping by flow cytometry in refractory cytopenia of childhood. Haematologica. 2015;100:315–23.
van Lochem EG, Velden VHJ, Wind JG, Marvelde JG, Westerdaal NAC, Dongen JJM. Immunophenotypic differentiation patterns of normal hematopoiesis in human bone marrow: reference patterns for age-related changes and disease-induced shifts. Cytometry B Clin Cytom. 2004;60B:1–13.
Wells DA, Benesch M, Loken MR, Vallejo C, Myerson D, Leisernring WM, et al. Myeloid and monocytic dispoiesis as determinated by flow cytometry scoring in myelodysplastic syndromes correlates with the IPSS and with outcome after hemopoietic stem cell transplantation. Blood. 2003;102:394–405.
Stachurski D, Smith BR, Pozdnyakova O, Andersen M, Xiao Z, Raza A, et al. Flow cytometric analysis of myelomonocytic cells by a pattern recognition approach is sensitive and specific in diagnosing myelodysplastic syndrome and related marrow diseases: emphasis on a global evaluation and recognition of diagnostic pitfalls. Leuk Res. 2008;32:215–24.
Chu SC, Wang TF, Li CC, Kao RH, Li DK, Su YC, et al. Flow cytometric scoring system as a diagnostic and prognostic tool in myelodysplastic syndromes. Leuk Res. 2011;35:868–73.
Tang G, Jorgensen JL, Zhou Y, Hu Y, Kersh M, Garcia-Manero G, et al. Multi-color CD34(+) progenitor-focused flow cytometric assay in evaluation of myelodysplastic syndromes in patients with post cancer therapy cytopenia. Leuk Res. 2012;36:974–81.
Reis-Alves SC, Traina F, Saad ST, Metze K, Lorand-Metze I. The impact of several phenotypic features at diagnosis on survival of patients with myelodysplastic syndromes. Neoplasma. 2010;57:530–6.
Lorand-Metze I, Califani SM, Ribeiro E, Lima CS, Metze K. The prognostic value of maturation-associated phenotypic abnormalities in myelodysplastic syndromes. Leuk Res. 2008;32:211–3.
Ribeiro E, Matarraz Sudón S, Santiago M, Lima CSP, Metze K, Giralt M, et al. Maturation-associated immnophenotypic abnormalities in bone marrow B-lymphocytes in myelodysplastic syndromes. Leuk Res. 2006;30:9–16.
Westers TM, Ireland R, Kern W, Alhan C, Balleisen JS, Bettelheim P, et al. Standardization of flow cytometry in myelodysplastic syndromes: a report from an international consortium and the European LeukemiaNet Working Group. Leukemia. 2012;26:1730–41.
Reis-Alves SC, Traina F, Harada G, Campos PM, Saad ST, Metze K, et al. Immunophenotyping in myelodysplastic syndromes can add prognostic information to well-established and new clinical scores. PLoS One. 2013;8:81048.
Kern W, Haferlach C, Schnittger S, Haferlach T. Clinical utility of multiparameter flow cytometry in the diagnosis of 1013 patients with suspected myelodysplastic syndrome: correlation to cytomorphology, cytogenetics, and clinical data. Cancer. 2010;116:4549–63.
Matarraz S, Lopez A, Barrena S, Fernandez C, Jensen E, Flores J, et al. The immunophenotype of different immature, myeloid and B-cell lineage-committed CD34+ hematopoietic cells allows discrimination between normal/reactive and myelodysplastic syndrome precursors. Leukemia. 2008;22:1175–83.
Xu F, Guo J, Wu LY, He Q, Zhang Z, Chang CK, et al. Diagnostic application and clinical significance of FCM progress scoring system based on immunophenotyping in CD34+ blasts in myelodysplastic syndromes. Cytometry B Clin Cytom. 2013;84:267–78.
Westers TM, van der Velden VH, Alhan C, Bekkema R, Bijkerk A, Brooimans RA, et al. Implementation of flow cytometry in the diagnostic work-up of myelodysplastic syndromes in a multicenter approach: report from the Dutch Working Party on Flow Cytometry in MDS. Leuk Res. 2012;36:422–30.
Lorand-Metze I, Pinheiro MP, Ribeiro E, de Paula EV, Metze K. Factors influencing survival in myelodysplastic syndromes in a Brazilian population: comparison of FAB and WHO classifications. Leuk Res. 2004;28:587–94.
Ribeiro E, Lima CSP, Metze K, Lorand-Metze I. Flow cytometric analysis of the expression of Fas/FasL in bone marrow CD34+ cells in myelodysplastic syndromes: relation to disease progression. Leuk Lymphoma. 2004;45:309–13.
Falco P, Levis A, Stacchini A, Ciriello MM, Geuna M, Notari P, et al. Prognostic relevance of cytometric quantitative assessment in patients with myelodysplastic syndromes. Eur J Haematol. 2011;87:409–18.
Porwit A, van de Loosdrecht AA, Bettelheim P, Brodersen LE, Burbury K, Cremers E, et al. Revisiting guidelines for integration of flow cytometry results in the WHO classification of myelodysplastic syndromes—proposal from the International/European LeukemiaNet Working Group for Flow Cytometry in MDS. Leukemia. 2014;28:1793–8.
Greenberg PL, Tuechler H, Schanz J, Sanz G, Garcia-Manero G, Solé F, et al. Revised international prognostic scoring system for myelodysplastic syndromes. Blood. 2012;120:2454–65.
Malcovati L, Della Porta MG, Strupp C, Ambaglio I, Kuendgen A, Nachtkamp K, et al. Impact of the degree of anemia on the outcome of patients with myelodysplastic syndrome and its integration into the WHO classification-based Prognostic Scoring System (WPSS). Haematologica. 2011;96:1433–40.
Schanz J, Tuchler H, Sole F, Mallo M, Luno E, Cervera J, et al. New comprehensive cytogenetic scoring system for primary myelodysplastic syndromes (MDS) and oligoblastic acute myeloid leukemia after MDS derived from an international database merge. J Clin Oncol. 2012;30:820–9.
Nakayama S, Yokote T, Hirata Y, Iwaki K, Akioka T, Miyoshi T, et al. An approach for diagnosing plasma cell myeloma by three-color flow cytometry based on kappa/lambda ratios ofCD38-gated CD138+ cells. Diagn Pathol. 2012;7:31.
Rimsza LM, Day WA, McGinn S, Pedata A, Natkunam Y, Warnke R, et al. Kappa and lambda light chain mRNA in situ hybridization compared to flow cytometry and immunohistochemistry in B cell lymphomas. Diagn Pathol. 2014;9:144.
Ogata K, Kakumoto K, Matsuda A, Tohyama K, Tamura H, Ueda Y, et al. Differences in blast immunophenotypes among disease types in myelodysplastic syndromes: a multicenter validation study. Leuk Res. 2012;36:1229–36.
Chantepie SP, Cornet E, Salaun V, Reman O. Hematogones: an overview. Leuk Res. 2013;37:1404–11.
Financial support: FAPESP, CNPq (INCTS 2008-57895/1), FAEPEX (proc 1208/11 Research fund of the University of Campinas) and MDS Foundation (Tito Bastianello Young Investigator grant 2009). Konradin Metze and Irene Lorand-Metze have a research grant from CNPq (proc. 307270/2010-6 and 302277/2009-9 respectively) We thank Fernanda G.P. Cunha and Felipe F. Rocha for their technical assistance.
The authors declare that they have no competing interests.
SCRA was responsible for flow cytometric analysis, participated in the statistical analysis and manuscript writing. FT contributed with the selection of patients, their clinical follow-up, and cytogenetic analysis. KM performed the statistical analysis and participated in the data interpretaion. ILM was responsible for the study design, interpretation of the results and final revision of the manuscript. This work is a part of the PhD thesis of SCR-A with ILM as the advisor (Post-graduate Course of Internal Medicine, University of Campinas). All authors read and approved the final manuscript.
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Reis-Alves, S.C., Traina, F., Metze, K. et al. Improving the differential diagnosis between myelodysplastic syndromes and reactive peripheral cytopenias by multiparametric flow cytometry: the role of B-cell precursors. Diagn Pathol 10, 44 (2015) doi:10.1186/s13000-015-0259-3
- Flow cytometry
- CD34+ cells
- B-cell precursors