From www.bloodjournal.org by guest on February 6, 2015. For personal use only. In Multiple Myeloma, Clonotypic B Lymphocytes Are Detectable Among CD19+ Peripheral Blood Cells Expressing CD38, CD56, and Monotypic Ig Light Chain By P. Leif Bergsagel, Anna Masellis Smith, Agnieszka Szczepek, Michael J. Mant, Andrew R. Belch, and Linda M. Pilarski Multiple myeloma (MM) is characterized by a plasma cell infiltrate of the bone marrow (BM). However, late-stage monotypic B cells have been detected in the blood. This work analyzes the effects of clinicaltreatment on late stage CD19+ B cells present in 752 blood samples from 152 MM patients. MM patients have 2 t o 8 times as many circulating CD19’ cells as do normal donors. Analysis of the Ig heavy chain (IgH) gene rearrangements using polymerase chain reaction indicates that the CD19+ population includes cells sharing the same clonotypic CDR3 region as is detected in the BM plasma cells, for patients analyzed during chemotherapy or in relapse. They are also monotypic as defined by their cytoplasmic or surface expression of lgK or A light chain. The light chain restriction is thesame as that of the BM plasma cells. Individual patients observed over 1- t o 2year periods exhibit considerable variation in the number of B cells present in blood; this number does not correlate with the concentration of serum monoclonal Ig. The monoclonal blood CD19+ cells are not eliminated byany of the chemotherapy regimensanalyzed and remain at high levels during transient remissions. Patients in the progressive phase of disease or in relapse have significantly higher numbers of B cells than do patients in transient remission or untreated patients. During periods when the quantityof blood B cells approaches normal, phenotypically their qualityis highly abnormal, with physical and phenotypic heterogeneity. Most B cells express CD45RO. a high density of CD38, and CD56 characteristic of late-stage B or pre-plasma cells. CD38h’ blood B cells had a cyclical presence. We conclude that monoclonal B cells in the bloodof myeloma patient populations include drug-resistant reservoirs of clonotypic cells that may underlie relapse. 0 7995 by The American Society of Hematology. M s i o n ~ . ’It~has ~ been suggested that the malignant stem cells in myeloma may be immature that colonize hernatopoietic microenvironments, including the Accumulating evidence implicates a circulating late-stage CD 19+ B cell in myeloma 10~’2-’1 and clonotypic rearrangements as defined by the BM plasma cells in myeloma have been reported among blood lympho~ytes.”~’~ A preliminary report indicates clonotypic sequences among purified CD19+ peripheral blood mononuclear cells (PBMCs).” Analysis of CD45 isoform expression on CD19+ cells in the blood and BM of myeloma patients indicates a heterogeneous continuously differentiating B lineage,’0,’2in contrast to other Bcell malignancies such as B-cell chronic lymphocytic leukemia (B-CLL), lymphoma, or hairy cell l e ~ k e m i a . ’ ~ ~ ’ ~ ~ ’ ~ Monoclonal rearrangements of the Ig heavy chain locus are detectable in blood from a proportion of patients 12.18,27 and mRNA encoding either K or A butnotboth light chains was detectable in myeloma PBMCS.’~A large proportion ofCD19’ cells in myeloma PBMCs have extensive DNA aneuploidy.I5,l6Unlike plasma cells or BM-localized B cells, and consistent with expectations for an invasive cell type, the monoclonal blood CD19+ cells express adhesion molecules, including CD1 lb,I3 a2p1, and a6pl integrin receptors for extracellular matrix,I4 selectins, and CD44.I’ For nearly all patients with myeloma, circulating CD19’ cells express functional multidrug transporter, p-glycoprotein 170.’5.21.28 The numberand phenotypic properties of CD19’ cells intheblood of myeloma patients, andtheir relationship to malignant plasma cells, were analyzed as a function of chemotherapeutic treatment and course of disease. We find clonotypic IgH rearrangements among CD19’ cells expressing cytoplasmic Ig at diagnosis, during therapy and off treatment. Thus, CD19+ B cells persist despite chemotherapy and, for those patients with apparently normal numbers, CD19+cellsin blood are phenotypically abnormal. ULTIPLE MYELOMA (MM) is a malignancy of the immune system characterized by accumulations of plasma cells in the bone marrow (BM), usually by a high concentration of monoclonal Ig in serum or urine and lytic bone lesions arising from osteolytic activity of plasma cellactivated osteoclasts.’ Although many patients respond to chemotherapy, nearly all eventually relapse and become refractory to further treatment.’ The measure of response to chemotherapy is a reduction in BM plasma cells, loss of the monoclonal Ig peak, and relief from bone pain and other symptoms. However, even though plasma cells are apparently eradicated from the BM by therapy and monoclonal Ig becomes undetectable by conventional assays, for nearly all patients the disease persists in an apparently cryptic com~ a r t r n e n t . ~The ’ ~ mean survival postdiagnosis is approximately 3 year^.'.^.^ Although MM is a cancer of the BM, the therapy-induced loss of BM plasma cells does not lead to long-term remis- From the Departments of Immunology and Oncology, University of Alberta, Edmonton, Alberta, Canada; and the Navy Medical Oncology Branch, National Cancer Institute, Bethesda, MD. Submitted February 28, 1994; accepted September 27, 1994. Supported by the National Cancer Institute of Canada with funds from the Canadian CancerSociety, and by The AlbertaCancer Board Research Initiatives Program. A.M.S. is the recipient of a fellowship from the Leukemia ResearchSociety and the Alberta Heritage Foundation for Medical Research. Address reprint requests to Linda M. Pilarski, PhD, Department of Immunology, University of Alberta, Edmonton, AB T6G2H7, Canada. The publication costsof this article were defrayedin part by page chargepayment. This article must therefore be hereby marked “advertisement” in accordance with 18 U.S.C. section 1734 solely to indicate this fact. 0 1995 by The American Society of Hematology. Oa)6-4971/95/8502-a)28$3.00/0 436 Blood, Vol 85, No 2 (January 15). 1995: pp 436-447 From www.bloodjournal.org by guest on February 6, 2015. For personal use only. CLONOTYPICBCELLS 431 IN MYELOMA 100 80 S 0 0 .-P 60 U) U) g :* ;*. a. 40 5a U- 0 20 c t E 1 a 28*2 31*1' 397 n = 98 31*1 257 I Untreated Treated Off Treatment Treatment Status of Myeloma Patients Fig 1. CD19' B cells in blood persist despite chemotherapy. Each symbol represents a single patient sample. The percentage of C D W cells actually detectedin PBMCs is presented here, in preference to absolute valuesin blood, becausethe percentage isa direct, unmanipulated data point.* P = .07 as compared with untreated patients. MATERIALS AND METHODS Patients. Patients with MM were observed for periods of up to 2 years, at monthly intervals, after informed consent was obtained. A total of 752 blood samples from 152 patients were analyzed for some or all of the parameters described in the Results. The majority of patients in all groups received a complete phenotypic analysis. A total of 14 patients were analyzed by CDR3 polymerase chain reaction (PCR). Of these, only 8 showed a single major IgH rearrangement among the purified BM plasma cells, consistent with other reports?3 which allowed identification ofa clonotypic rearrangement for comparison with IgH rearrangements in purified blood B cells. Phenotypic information was maintained in a set of linked databases for clinical and research data using dBASEIV (Borland, Scotts Valley, CA). The patients included 50 untreated (at diagnosis), 43 on melphaladprednisone (MiP), 42 on vincristine/ adriamyciddexamethasone (VAD), 9 on biologic response modifiers or IFN plus interleukin-2 (IL-2), and 68 off chemointerferon (IFN) therapy. Because most patients were observed for prolonged periods of time, a single patient usually appears in several of these groups. Patients on intermittent chemotherapy were studied at least 4 weeks after their latest treatment. The definition of clinical parameters was as described by Durie and Salmon.' Seventeen normal, healthy volunteers were analyzed at single time points as controls. Patients were designated as off treatment 2 months after their last cycle of chemotherapy. However, most patients in this category had been off treatment for longer periods of time. Purijication ofPBMCs. Venous blood samples were drawn into heparinized vacutainer tubes and the PBMCs were isolated on a Ficoll-Paque (Pharmacia, Dorval, Quebec, Canada) density gradient. Cells harvested from the interface were washed twice inRPM1 (GIBCO, Grand Island, NY) and resuspended in phosphate-buffered saline, including 2% fetal calf serum (HyClone Labs, Logan, UT). Methods for depletion of adherent cells were carefully avoided, because the abnormal CD19+ cells in myeloma have adherent properties and are depleted by such procedures.'* Antibodies. IgGlFITC,IgGlPE, IgGZFITC, and IgG2PE were from Southern Biotech (Birmingham, AL). LeulSPE (CDllb), Leul7PE (CD38), J5FITC (CDlO), and HNK-l (CD56) were purchased from Becton Dickinson (San Jose., CA). From Coulter (Hialeah, FL), we purchased B4-FITC (CD19) and B1-RD1 (CD20). Monoclonal antibody (MoAb) FMC63 (CD19) was from H. Z ~ l a ? ~ UCHLl (CD45RO) from P. Beverley,Mand PCA-1 from K. Anderson." For detection of circulating CD19' B cells in the blood of myeloma patients, either FMC63 or the commercially available B4 MoAb (Coulter) gave comparable results, but these cells were not reliably detected with Leu-l2 (Becton Dickinson) in our hands. However, others have reported large numbers of CD19+ cells in PBMCs from myeloma patients using Le11-12.~'They were not reliably detected with phycoerythnn (PE) conjugates of CD19 MoAbs, probably reflecting steric hindrance from these bulky phycobiliproteins. MoAbs to Ig light chain used in immunohistochemistry were from the American Type Culture Collection (Rockville, MD); those used for immunofluorescence (IF) were F(ab), fragments conjugated to fluorescein isothiocyanate (Southern Biotech). Goat antihuman 10-PE and goat antimouse Ig-PE were from Southern Biotech. Two-color ana' three-colorimmunojluorescence. A two-color fluorescence staining procedure was used for the study of surface marker expression as previously PBMCs were incubated with antibodies to be detected by indirect IF (isotype controls, Table 1. Circulating B Cells in Blood Do Not Decrease in Number After Chemotherapy Treatment Percentage of CD19' in PBMCs Percentage of CD19' XlO-'/L of Blood 28 2 2.8 300.30 2 1.9 36 2 1.5t 33 2 3.3 28 2 1.6 6 2 1 0.44 2 0.06 2 0.02* 0.43 2 0.03 0.33 -C 0.03* 0.32 -t0.15 0.03' 0.06-0.24 Small B Cells xlO-'R of Blood Cells Large B xlO-'/L of Blood mlg (glLI 0.26 42 t 0.04 t 280.02 0.34 24 t 0.04 0.19 2 0.01 0.23 t 0.02 1.82 2 4.9 2 1.9t t 3t 29 2 0.38* 29 t 2.3t Lymphocytes x lo-% of Blood ~~~ Untreated MIP VAD IFNIIL-2 Off Tr Normal 0.20 0.12 0.07 0.14 0.04 2 0.20.01' 2 0.02$ 2 0.03 2 0.02 -C 2 0.17 0.98 -t 0.06t 1.38 -t 0.11 0.81 2 O.06t 1.19 -t 0.08t 1.0-4.0 Values are the mean 2 SE. Unmarked values are not significantlydifferent from the untreated values.The number ofCD19+ cells in blood was calculated as the (white blood count IWBCI x % lymphocytes x %CD19+ in PBMCs). The number of lymphocytes was(WBC x % lymphocytes). Abbreviation: Off Tr, chemotherapy discontinued. * P S .07 as compared with untreated patients. t P S .03 as compared with untreated values. P = ,003 as compared with untreated values. * From www.bloodjournal.org by guest on February 6, 2015. For personal use only. BERGSAGEL 438 A l 1 1 AL .Id -MR1 I n t e n s i t y of fluorescence B " B Cells lg Expression: Log Fluorescence 600bp 500bp 400bp 300bp 200bp 1 OObp Fig 2. Expression of CD19 on myelomaPBMCs and expression of CD20 on theCD19' subset of PBMCs. (A) PBMCs were stained with CDl9-FITC and CD2O-RD1 (-1 or an isotype-matched lgG2 MoAB (-4. Row 1 is the staining by CD19-FITC and the marker bar (R11 indicates the cells considered t o be positive for CD19 and the electronic gate definingCD19' cells. Row 2 is the staining byCD2O-RDl on PBMCs gated for CD19(R1). Ungated (CD19) and gated (CD201 histograms are from 3 representative patients. Staining by FMC63FlTC and by BCFITC was nearly identical. (B) RT-PCR analysis using CD19 primers t o amplify mRNA from freshly isolated and sorted B or T cells from the same patient. PCR was performed on RNA from 10' cells. (C) CD19+ PBMCs express lg. Files were gated for CD19' cells as indicated in the top panel and the expression of lg plotted as histogram. (...l Staining with goat antimouse Ig-PE (control). (-) Staining of CD19' PBMCs with goat antihuman Ig-PE. (- .. -1 Staining of plasma cells with goat antihuman lg. The values within each peak indicate the proportionof gated CDl9+ PBMCs or plasma cells with that intensity of staining. Similar results were obtained with PBMCs from 10 other patients; in all 10, the proportion of B cells expressing detectable l g was 80% or higher. From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 439 CLONOTYPIC B CELLS IN MYELOMA 50 T 40 U g 30 a + 2 :: 20 K 10 0 Unt Prog Relapse > l Remission Relapse Fig 3. Patients who have relapsed one or more times have the highest proportion ofCD19* B cells in blood. Prog, progressing. As compared with untreated values, all relapsed patients hadP = .W1, tho- relapad more than l time had P = .ooo5, andthoseprogressing hadP = .03. Patients in transient remission were not significantly different from untreated patients. UCHLl, or PCA-l), washed, blocked with mouse Ig, and stained with a direct conjugate of B4-FITC or FMC63FITC. A double-direct IF procedure was used for staining of cells with PE-conjugated isotype controls, BlRDl, LeulSPE, or Leul7PE and FMC63FITC. Stained cells were washed twice and fixed in 1% formalin for flow cytometric analysis. Analysis of IF. Samples were analyzed using a FACScan (Becton Dickinson). Red blood cells and dead cells were excluded by electronic gating on forward angle light scatter and files of 10,000 to 20,000 cells were collected. Files were electronically gated for CD19+ cells and the expression of the second MoAb was plotted as a histogram. In all cases, staining with a specific MoAb was compared with its appropriate isotype-specific control, with identical electronic gates for B-cell subsets. To maintain a consistent evaluation of the intensity of staining among different patients, a precise definition was used. In all cases, on a log scale, the intensity of staining was categorized as moderate (between 10' and 10') or high (staining greater than 10'). CD19' cells were also evaluated for their physical properties as measured by forward (FALS) and side angle scatter (SSc), as previously des~ribed.'~.'~,'~ Cells designated as small were those with SSc less than channel 400, whereas those designated as large had SSc greater than channel 400 on a linear scale. For most patients, FALS was also increased among the large cells. Som'ng. SOmng was on an ELITE flow cytometer (coulter). PBMCs were stained with FMC63-FI'K or CDllb-PE, followed by sorting for staining greater than the isotype-matched control. Sorted B cells were r e p lysates for DNA analysis or concentmted, counted,and used to p cells cytospinsforimmunohistochemistry. PCA-I+ cIgh'BMplasma were sorted for PCR analysis of CDR3 clonotypicm g e m e n t s . Ig heavy chain gene analysis. PCRwasused to amplify VDJ rearrangements from blood B cells sorted for expression of CD19 and, in some cases, sorted into a CD19 small subset and a CD19 large subset. For those patients tested, the majority (80% to 100%) of CD19+ B cells expressed detectable cytoplasmic Ig. BM plasma cells were purified by sorting for cells which coexpressed the plasma cell marker PCA-l and a high density of cytoplasmic Ig (cIg). IgH$ngerprinting. Whole cell lysates of the sorted cell populations were prepared22and resuspended at a concentration of 1,OOO cells/pL. One microliter of the cell lysate was used in a 25-pL PCR reaction in 10 mmoVL Tris, pH8.3, 50 mmoVLKCI, 2 mmoVL MgC12, 200 pmoVL dNTP, 0.025 U/pL Taq polymerase (Amplitaq; Perkin Elmer, Branchburg, NJ), 0.2pmoVL FR2a (codons 42-47 TATGAATTCGGAAAGGGCCTGGAGTGG),and 0.2 pmoVL JH1 (codons 114-109 ACGGGATCCACCTGAGGAGACGGTGACC), with cycling 25 times between 94°C for 30 minutes, 52°C for 30 minutes, and 72°C for 30 minutes. From this reaction, 0.5 pL was placed into a second-stage PCR in a 5-pL reaction performed as above, with the oligonucleotides being 1 pmoVL FR2a and 0.1 pmoV L 32PATP end-labeled JH2 (codons 110-103 ACGGGATCCGTGACCAGGGTNCC'ITGGCCCCAG), with cycling for 20 times. Two microliters of this reaction was electrophoresed on a 6% denaturing polyacrylamide urea gel and the gel was exposed to XAR film(Eastman Kodak, Rochester, NY). Sequencing. The CDR3 PCR products were amplified as above and purified from an agarose gel using Promega Magic PCR Preps (Promega, Madison, WI). The nucleotide sequence was determined using end-labeled oligonucleotides FR2 and JH2 with Promega's fmol PCR sequencing kit (Promega). Allele-specific oligonucleotides AS0 were designed based on the nucleotide sequence and synthesized by Genosys Biotechnologies Inc. (The Woodlands, TX). CDR3 PCR and AS0 Southern blot. Using the same conditions as above, 1 pL of the cell lysate was amplified with oligos FR2a and JH1 for 30 cycles. From this reaction, 0.1 pL was placed ina secondstage PCR under the same conditions, with oligos FR2b [codons 6469 ATGGAATTCAGGGC(C/A)G(A/G)(T/G)TCACCAT]and JH2 for 30 cycles. Ten microliters of this reaction was electrophoresedon a 4% Nusieve GTG agarose gel containing ethidium bromide. The DNAwastransferred to a Nylon filter by Southern blotting. The Nylon filters were hybridized tothe patient specific end-labeledAS0 in 5X SSC, 1% sodium dodecyl sulfate (SDS), and 20% formarnide at 42°C for 4 hours, and then washed three times in 5X SSC, 1% SDS at 22°C for 5 minutes and once at 42°C for 5 minutes. The filter was exposed to XAR film for 2 hours at -70°C. Immunohistochemistry. Cytospins were air-dried, fixedin acetone, and stained with Wright's stain for morphologic evaluation, followed by staining with anti-^ or anti-A to determine light chain expression. Cells were incubated with primary antibody for 60 minutes at room temperature followed by two washes in phosphatebuffered saline (PBS). Horseradish peroxidase conjugated to goat antimouse Ig was added for a further 15 minutes of incubation at room temperature. Freshly prepared DAB (3-3'diaminobenzidinetetrachloride; Sigma, St Louis, MO) in PBS containing 0.008% hydrogen peroxide was added to cells for 4 to 5 minutes and the degree of staining was determined by comparison to isotype-matched controls. Reverse transcriptase-PCR (RT-PCR) for CD19 mRNA. Based on the sequence of the CD19 gene,33.34primers for RTPCR were designed by and obtained from Dr Tom Tedder (Duke University, Durham, NC). Using Trizol according to the manufacturer'sdirections(GIBCO,Burlington,Ontario,Canada), RNA was prepared from populations of sorted B cells and from sorted T cells of the same patient, collected at the same time in a double immunofluorescence sort, to serve as a negativecontrol. After purification, 1 pg of RNA was reverse transcribed using SuperScript reverse transcriptase (GIBCO BRL) and universal primer oligodT,, (BoehringerMannheim,Laval, Quebec, Canada)ac- From www.bloodjournal.org by guest on February 6, 2015. For personal use only. BERGSAGELET AL 440 BM BL BM BL BM BL PCA1+ CD19+ PCA1+ CD19+ PCA1+ CD19+ large small large small -p J Fig 4. Clonotypic IgH rearrangements defined by BM plasma cells characterize blood B cells in myeloma: IgH fingerprint analysis. CDR3 VDJ rearrangements were analyzed by PCR on 3patients. Hemi-nested PCR was performedas described using a radiolabeled JH2 primer and run on denaturing6% acrylamide gel. The samples of BM and blood (BL) were sorted for the indicated populations. (Left panel) Patient no. 1, off treatment (tr) relapse. This patient was diagnosed in early 1992 and responded to M/P followed by IFN maintenance therapy. Massive relapse occurred in late 1993, at which time the BL and BMsamples in the figure weretaken. Sixty-five percent of total BM were PCA-l' cells and 24% of PBMCs were CD19'. ASO-PCR confirmed the clonotypic band for this patient. (Middle panel) Patient no. 2, t r after relapse. This patient was diagnosed in early 1992, responded t o MIP, and relapsed in late 1993. M/P hadbeen reinitiated for 1 month with noresponse at the time this sample was taken. Sixty-three percent of BM werePCA-l' and 20% of PBMCs were CD19'. The single band detectedamong the large B cells for this patient was confirmed t o be clonotypic with ASO-PCR. (Right panel) Patient no. 3,Tr, after relapse. The patient was diagnosed in late 1988, responded t o M/P, and remained on M/P plus IFN in a stable condition until late 1993, at which time the disease escaped plateau phase. M/P hadbeen reinitiated for 3 months with symptomatic improvement at the time these samples were taken. Ninetythree percent of BM werePCA-1' and 10% of PBMCs were CD19'. The clonotypic band was included among the ladder of bands detected for this patient as confirmed by probingwith the AS0 (Fig 5). cording to the manufacturer's instructions. Briefly, RNA was incubated with the primer for 10 hours at 70°C and chilled on ice and the buffer, DTT, and enzyme were added. The reaction tube was placed at 40°C for 1 hour followed by heating for 3 hours at 100°C. PCR was performed under standard conditions. Briefly, 2 pL of cDNA from the reverse transcriptase reaction was added to 48pL of PCR buffer (GIBCO BRL; 1.5 mmol/L MgCL2)mixed with primers for CD19 crossing two introns (a gift of Dr Tom Tedder) and 1 Ulreaction tube of TAQ polymerase (GIBCO BRL): 35 cycles of 30 seconds at94°C. 30 seconds at55°C. and 45 seconds at 72°C wasperformed on the PCR Thermal Cycler Perkin Elmer 9600. PCR product was analyzed on a 2% agarose gel in Tris/boric acid/EDTA buffer, soaked in ethidium bromide, and visualized under UV light. Sfaristical evaluation. Values from patients on chemotherapy or off treatment were compared with those from untreated patients using a two-tailed t-test. RESULTS CD19+ B cells persist in blood despite chemotherapy. Figure 1 shows the distribution of CD19' cells in individual PBMCs as a function of treatment status. There is a broad range of values in all treatment categories andthemean values are comparable for all groups (Table l). Although for any given patient an increased percentage of CD19' cells is always found at some time points throughout the disease progression, the numerical value is not always abnormal, as indicated by the values below 15%, the normal range'' (Fig From www.bloodjournal.org by guest on February 6, 2015. For personal use only. CLONONPIC B CELLS IN MYELOMA 441 Table 2. Nucleotide Sequence of IgH VDJ Rearrangements Amplified From BM FR3 COR3 JH 1 TGTACG ..GGGGGCAACTT .............. CTGGGGC 2 TGTGTGAGA.TGGGTCAGAGGGGTCAATCCTCCCTTCAT.TGAAGACTTCCAGAA CTGGGGC 3 TGTACGAGA.GATCAAGATGACTACGGTGACTACGGGAC ...CTTTAACTC CTGGGGC CODONS 92 104 The sequence is given for the patients referred to in Figs 4 and 5. The ASOs were synthesized based on the complement of the regions underscored. l). However, as will be detailed later, these quantitatively normal B cells are phenotypically abnormal. In all treatment categories, the majority of samples included an abnormally high proportion of CD19' B cells. Figure 2 (top panel, row 1) shows the CD19 MoAb staining of myeloma PBMCs and the marker bar indicates those cells recorded in Fig 1. These CD19' PBMCs expressed CD19 mRNA, as detected by RTPCR analysis of sorted CD19' B cells, the absence of CD19 mRNA from T cells sorted from the same PBMCs patient samples (Fig 2, bottom left), and the expression of Ig by the CD19' population (Fig 2, bottom right). PBMCs gated for CD19 expression coexpress CD20, including CD19' CD20hi andCD19' CD20'"'md subpopulations (Fig 2, top panel, row 2). Table 1 gives the absolute number of CD 19' cells in blood and the mean percentage of lymphocytes. The values of CD19' B cells in PBMCs range from 0.33 to 0.63 X 109/L of blood. These values are above the normal range for B cells, even though many patients are lymphopenic. Untreated patients at diagnosis have 0.44 X lo9 B cells/L of blood, with 24% of lymphocytes in blood being CD19' cells (Table 1, line 1). Patients treated with M P , on second-line therapy with biologic response modifiersIFN andor L-2, or off therapy have the lowest absolute number of blood B cells (0.3 to 0.33 X 109/L) (line 6). 1 CD19+ CD19+ 3 2 Unrelated Unsorted Previous workhas indicated that monoclonal B cells in the blood of nearly all myeloma patients can be subdivided into a set with low SSc (designated "small") and a set with high SSc (designated "large") that is not found in normal donors. The subset of small B cells is phenotypically heterogeneous.'n.'2.'3)The large PBMC B cells are a relatively homogeneous In untreated patients, approximately half of the circulating B cells are small B cells and half are large late-stage B cells (Table l , columns 4 and 5 ) . For patients treated with MiP or with VAD, the number of small B cells was significantly decreased as compared with untreated patients ( P c .07). The number of large B cells did not change with treatment. The B cells in patients treated with biologic response modifiers ( I F N or IFNAL-2) or patients off treatment were not significantly different from those in untreated patients. The number of circulating B cells was compared among patient groups defined by their disease status (Fig 3). A significant difference in the percentage of CD19' B cells in PRMCs was detectable, with the lowest values among those patients in transient remission and the highest in patients with progressive disease or those who have had one or more relapses. CD19' cells in blood of myeloma patients express clonotypic IgH VDJ rearrangements. Hemi-nestedPCRwas used to compare IgH rearrangements in sorted populations of blood CD19+ cells with sorted PCA-l' plasma cells from the BM. PCR using consensus oligonucleotides to the IgH variable region framework 2 (FR2) and the IgH J segment (JH) genes amplifies rearranged heavy chain genes, but not germline heavy chain genes (because germline FR2 and JH are too distant to be amplified). Because of different D gene lengths, and N region diversity, the length of the VDJ rearrangements amplified varies within a range of about 48 nucleotides, changing in increments of three nucleotides (be- BM Unrelated PCA1+ CD19+ CD19+ CD19+ BM Unrelated Unsorted CD19+ CD19+ - 232 bp - 192bp - 118 bp _. . . - 232 bp - 192 bp - 118 bp Fig 5. Clonotypic IgH rearrangements defined by BM plasma cells characterize blood B cells in myeloma: nested CDR3-PCR probed with an ASO. Forthe same 3 patients as in Fig 4, although with samples obtained at a later date, the VDJ rearrangementswere amplified by nested CDR3-PCR and electrophoresed on an ethidium bromide stained agarose gel (top panels). These rearrangementswere transferred to a nylon filter by Southern blotting, probed under stringent conditions with an end-labeled ASO, unique for each patient, and exposed to XAR film (bottom panels). For patient no. 2, CD19+ B cells were purified from blood at two time points after the sample analyzed in Fig 4. For all 3 patients, samples were collected and subjected to flow cytometric sorting at approximately 2- to 3-month intervals. From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 442 Fig 6. Circulating CDl9+ B cells express lg light chain. Cytospins were made from PBMC B cells of a patient with IgGK myeloma. Slides were stained with either anti-K or anti-AF(ab), fragments conjugated to FITC and examined usingconfocalmicroscopy. B cells were scanned at 1,400~power at 512 x 512 resolution. The left image is of small B cells with predominantly surface staining and low cytoplasmic staining with anti-K. The right image is of a large B cell with strong cytoplasmic staining forK light chain. A variety of gradations of staining patterns between these two extremes were always detected among the CD19' blood B cells. No staining was detectable for cells from this patient stained with anti-A. cause the majority of rearrangements preserve an intact open reading frame). When electrophoresed on a high resolution sequencing gel, the rearrangements present in a polyclonal B-cell population thus appear as a ladder of approximately 16 bands, spanning 48 nucleotides. For a monoclonal B-cell population, such as purified BM plasma cells from a patient with myeloma, only a single rearrangement should be ampli- BERGSAGEL ET AL fied. In 8 patients, we amplified a unique rearrangement from their BM plasma cells, and we examined their blood CD19' cells by Ig fingerprinting. Figure 4 shows the result of hemi-nested IgH fingerprinting analysis in blood B cells and BM plasma cells for 3 of the 8 patients, chosen to reflect the heterogeneity in the amplification patterns observed. From the blood CD19' cells of the patient in the left panel, a single rearrangement of exactly the same size (222 bp) as that in the BM was amplified. The rearrangement amplified from the peripheral blood was sequenced and was identical to that in the BM, without evidence of somatic mutation. This is evidence of both clonotypic B cells in the CD19+ population, and a relative absence of other B cells (although all the cells in this population expressed Ig; Fig 2). This does not necessarily mean a complete absence of nonclonotypic B cells, because the hemi-nested PCR may greatly amplify small differences. We have not determined at what level a clonal rearrangement, in the presence of polyclonal rearrangements, will be amplified as a single band without evidence of a polyclonal ladder. For the patient in the middle panel, blood B cells were sorted into the small and large subsets: from the large B cells, only the clonotypic rearrangement (258 bp) was amplified; from the small B cells, a polyclonal ladder of rearrangements was amplified. For the patient on the right panel, many rearrangements were amplified from both the small and large B-cell subsets. Although a rearrangement(s) of the same size as the clonotypic one (252 bp) is evident in both populations, in the presence of so many other rearrangements, one cannot conclude that there are clonotypic cells in these populations. Therefore, the rearrangements amplified from the BM were sequenced and ASOs were synthesized (Table 2). To confirm the presence of patient-specific clonal rearrangements in the blood CD19' cells, all of therearrangements in a sample were amplified using nested CDR3 PCR (Fig 5). The top panel shows an ethidium bromidestained agarose gel of the nested PCRs from the same patients as in Fig 4, from samples collected at a later time point. This demonstrates that there are IgH rearrangements in all samples. To confirm thatthe amplified product includes clonotypic sequences, these rearrangements were hybridized to an end-labeled patient-specific A S 0 under stringent conditions so that only identical rearrangements should hybridize. The lower panel shows that clonotypic rearrangements are detected among the rearrangements in unsorted blood, and in CD19' cells, but not in the CD19' cells of an unrelated individual. Because this method analyzes DNA, as opposed to RNA, one need not beconcerned that a rare contaminating plasma cell will inordinately influence the result, there being only a single DNA rearrangement per diploid cell. The same results were obtained using ASO-PCR (ie, using the A S 0 in the PCR reaction with FR2); however, the sensitivity of ASO-PCR is theoretically much greater, andcoulddetect even a very rare cell. By amplifying all of the rearrangements in a sample there is no (or a least very little) selection imposed by the PCR. One can then ask what fraction of the amplified rearrangements are clonal. Although not quantitative, in relative terms a much greater proportion of amplified From www.bloodjournal.org by guest on February 6, 2015. For personal use only. CLONOTYPIC IN MYELOMA 443 Table 3. Small and b r a e CD19+ B Cells Are PhenotMicallv Abnormal in N 4 v Diaanosed Patiants and Thore on or off ChernotheraDv CD19 Small CD19 Large Phenotype Unt Tr off CD20 CDlO CD45RO CD1 bh' 1 PCA-l CD38h' CD56 61 t 7 33 2 17 61 t 7 3 2 1 45 t 13 16 2 3 24 2 14 52 2 6 47 2 12 53 t 4 17 2 7 50 2 14 12 2 21 -+ 12 57 t 5 37 i 11 4924 12 2 9 53 2 10 20 2 21 -+ 8 * * Unt 81 98 82 78 76 46 76 27 i2 t7 2 10 i 14 2 7 t 10 Off Tr 76 2 6 92 i 3 88 -c 3 85 2 8 76 2 9 46 -t 5 66 i 13 80 91 85 70 77 42 47 -t 4 i3 2 2 2 3 i8 i3 t 11 PBMC samples were stained with CD19 together with MoAb to the indicated marker in two-color immunofluorescence. Files were gated for CD19' cells and the expression of the marker was plotted as a histogram. Cells were considered to be positive only if the staining exceeded that of an identically gated isotype control MoAb. For CD1l b and CD38, only the highest density of expression is enumerated here (staining as indicated in the Materials and Methods). For the majority of cells, staining with CDlO and PCA-1 was generally at moderate intensity: staining with CD20,CD45RO. and CD56 was moderate to high as defined in the Materials and Methods. Values in the indicated treatment group or between different types of therapy were notsignificantly different from each other or from untreated values. rearrangements are clonal for patients no. 1 and 2 than, by comparison, for patient no. 3, for whom only a minority of the products in the band hybridize to the patient-specific AS0 probe. Patient no. 3 has had a prolonged plateau phase perhaps related to the relative paucity of clonotypic B cells (Fig 5) and the apparent presence of polyclonal B cells (Fig 4). Although clearly heterogeneous and including variable proportions of apparently polyclonal B cells in some patients and some subsets of B cells, clonotypic CDR3 sequences were nevertheless consistently detected at multiple time points during and after treatment in all patients tested and, for some patients, were detected in all subsets of B cells analyzed. In a total of 5 of the 8 patients, a single clonotypic rearrangement was amplified from the blood B cells or large/ small B-cell subsets on IgH fingerprinting, indicating clonotypic involvement. In all 8 patients clonotypic rearrangements were detected in the blood B cells or B-cell subsets using one or more technique of IgH fingerprinting, nested CDR3-PCR probed with an ASO, and ASO-PCR. B cells taken from the same patient over a 2- to 4-month period consistently exhibited the same clonotypic band. Purified T cells from the patient taken at the same time and B cells from an unrelated individual did not contain the clonotypic rearrangement. CD19+ cells in blood of myeloma patients have restricted light chain expression. To confirm Ig gene expression, cytoplasmic Ig light chain was evaluated in either sorted B cells or in total PBMCs. Cytospins were stained with either anti-K or anti-A, followed by microscopic examination. Samples were also evaluated using confocal microscopy of sorted B cells stained with fluorescent anti-light chain. Figure 6 shows representative examples of the small B cells with predominantly surface staining (Fig 6A) and large B cells with strong cytoplasmic staining (Fig 6B). Parallel staining with the opposite anti-light chain reagent gave no fluorescent staining. In 13 of 13 patients analyzed, sorted CD19+ B cells were positive for either K or A but not both, and the light chain expressed was the same as that for the monoclonal serum Ig or urine protein. The light chain type was the same for blood and BM B cells. Three patients were analyzed at two to three time points with consistent light chain restriction. For sorted B cells from all patients analyzed, the majority of B cells expressed cIg, and the intensity of staining with anti-light chain was heterogeneous, ranging from barely detectable to relatively intense (comparable to the fluorescent staining shown in Fig 6) but less than that of BM plasma cells, consistent with our phenotypic characterization of this population as heterogeneous and comprising a range of Blineage differentiation stages.1°,12Finally, the patient PBMCs analyzed in other studies for monoclonal Ig rearrangements, expression of light chain mRNA, or expression of Ig were also part of this s t ~ d y , " - ~ ~providing . ' ~ * ~ ~confirmation of Ig monoclonality for a total of approximately 60 patients. CD19+ PBMCs are phenotypically abnormal, expressing CD38, CD.56, and other antigens not detected on n o m 1 B cells. A significant proportion of CD19' PBMCs expressed both CD38 and CD56 (Table 3). Figure 7 shows representative histograms for the staining of CD38 during and after chemotherapy (Fig 7A), and of CD56 (Fig 7B), on CD19' PBMCs in myeloma. Among subsets of CD19+ cells gated for granularity (SSC; Table 3), for the majority of patients, the small B-cell subset expressed CD45RO and PCA-1, unlike normal B cells, but had only minor expression of CD56 (moderate intensity) or expression of ahigh intensity of CD38. The large B cells coexpressed CD19 and CD20, as expected for B cells. As previously shown with a smaller cohort, the majority of large B cells were CDlO+ CD45RO+ CD1 lbhiPCA-l', and are here shown to express a moderate intensity of CD56 and nearly half express a high intensity of CD38 (Fig 7 and Table 3). Overall, although clearly heterogeneous and including multiple B-cell differentiation stages, no significant differences in phenotype of MM blood B cells were found between different treatment groups. Because normal PBMC B cells do not express CDlOPCA-l, CD38hi,C D l l b ~ CD56, , or CD45R0,25Table 3 shows that numerically normal CD19' populations in blood in all cases include phenotypically abnormal cells. The majority of small B cells, the subset most comparable to normal B cells in its physical properties (FALSISSC), are qualitatively different From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 444 BERGSAGEL E T AL from and considerably more heterogeneous than normal B cells. Temporal changes in CD1 9+PBMCs occur during chemotherapy and over the course of disease but do not correlate with mZg levels. Individual patients were observed over time to evaluate the number of blood B cells together with clinical parameters. The patterns for 2 representative patients are shown in Fig 8. In all patients the number of B cells varied over time, as measured by the percentage of PBMCs or by the number in blood. For most patients, the number of B cells was relatively high at diagnosis and tended to increase or remain stable throughout chemotherapy, with periods when the level increased substantially (as shown in Fig 8). These increases did not correlate with increased monoclonal Ig, but would not be expected to do so. mIg is a measure of plasma cell tumor burden, and would not be expected to correlate with the numbers of PBMC B cells that have not yet acquired the capacity for a high rate of Ig secretion. For patient no. 1, the number of B cells decreased transiently after cytoreductive therapy and transplantation, but recurred within a few months posttransplant. The analysis of patient no. 2 began 2 years postdiagnosis after relapse and treatment with W. For this patient, the number of B cells appeared to increase with the cessation of therapy and with relapse, but decreased with therapy. The B cells from both patients were shown to be monotypic by analysis of light chain mRNAI3 andor of cytoplasmic Ig. A cyclical pattern of CD19+ B-cell levels was seen in 30 of 40 patients analyzed at multiple time points, including the period when chemotherapy terminated. Six of 40 patients maintained a high expression of CD19+ B cells throughout, and 4 of 40 had decreased CD19' levels after initiation of therapy that have not yet recurred to high levels. Cyclical presence of CD38"' B cells in blood is consistently detectable for most patients. A high density of CD38 (intensity of staining greater than lo2, Fig 7A) appears only late in the differentiation towards plasma cells and isnot seen on normal B cells in a d ~ l t s . The ~ ' percentage of CD38h' B cells was plotted over time for individual patients at the indicated month postdiagnosis (Fig 9). The percent of CD19+38hiB cells increased with the initiation of chemotherapy (month 1) and continued to increase for several months. Levels became depressed for a brief interval posttreatment (months 5 and 6) and then increased again (months 8 and I I I i l 101 102 103 Month I - 2 104 loo lo1 lo2 lo3 lo4 Month 5 - 7 C D 3 8 lmmunofluoresence CD56 l m m u n o f l u o r e s e n c e Fig 7. CD19*PBMCsexpress CD38andCD56. PBMCs were stained with CDl9-FITC and either CD38-PE or IgG1-PE in doubledirectimmunoffuorucence (A), or with CD66 or lgG1 M o b s followed by goat sntimouse IgPE in double direct/indirect immunofluorescence (B). (A) Expression of CD38 on CDl9' PBMCs from3representative myelomapatientsearlyduring chemotherapy and at a later point duringor after chemotherapy. (B) Expression of CD56on CDl9+ PBMCa from 3 representative patients. Files were gated for CD19+ cells and the expression of CD38 or CD58 plotted as a hintogram I-) in comparison to an identically gated isotypematched controleliquot ( - 4 For (A), the dashed vertical line indicaten mining at intensity of W . Cells with an intensity of staining above this point are d d g nated as CD38"'. From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 445 CLONOTYPIC B CELLS IN MYELOMA CD19+ x lO*/L Blood 70 IA X I o'8 c 0.6 50 40 0.4 30 20 0.2 10 n n v 9/91 11/91 12/91 1/92 2/92 3/92 5/92 6/92 9/9210/9211/92 2193 Date: Patient l % CDl9r x 10e/L Blood or MIg W L ) B 0.6 0.5 80 0.4 40 0.3 0.2 20 0.1 ,. U- specific oligomer PCR, and sequence analysis. As expected, and providing a negative control for the PCR reaction, clonotypic IgH rearrangements cannot be amplified from purified T cells derived from the same PBMCs as the CD19+ B cells. The rearranged Ig genes are functionally expressed in CD19' B cells as evidenced by the presence of low to moderate amounts of monotypic cytoplasmic Ig light chain. As defined by physical parameters, CD19+ PBMCs include a small and a large subset, both of which are predominantly late-stage CD19+20+B cells, previously shown to coexpress CD24."." Many of the large B cells coexpress CD56 and a high density of CD38. Although distinguished from plasma cells by the extent of Ig expression, by phenotype, and by morphology,L0~L3~L5~L9~20~28 these circulating CD19+ populations include cells within the malignant lineage as defined by the presence of clonotypic VDJ rearrangements with a sequence identical to that of the BM plasma cells, although there is as yet no direct evidence to indicate that they are themselves malignant. Clonotypic rearrangements were detected among the VDJ rearrangements amplified from the purified B cells, or Bcell subsets in all 8 informative patients, confirming the presence of clonotypic cells and, in some samples, a relative absence of nonclonotypic B cells. The best way of quantitating the frequency of clonotypic B cells relative to all B cells is by probing a nested CDR3 PCR, which amplifies all rearrangements, with an ASO. These data suggest that in some patients the clonotypic cells represent a majority of all B cells, and in others a minority. Further study is required to determine which B-cell subsets are predominantly clonal and how this correlates with a patient's clinical course. 9/90 10/90 7/91 6/91 12/91 1/92 4/92 9/92 12/92 2/93 n- Date: Patient 3 Fig 8. The number of CD19+ cells in blood varies with treatment and as the disease progresses,but remains high when mlg levels are reduced. Eachplot represents the results for 1individual patient over the indicated time period. Patient no. 1 was diagnosed as MGUS in 1989 and was diagnosed as stage 2A myeloma in November 1991at age 45; VAD treatment was initiated. VAD was completed in May 1992. The patlent was clinically asymptomaticand BM was harvasted for an autologoustransplant in November 1992.He remains clinically disease free. Patient no. 2 was diagnosed in November 1988 with symptomatic stage 2A myeloma at age 82. M/P was initiated in April 1989 for 6 uycles. He relapsed in May 1990 and again in December 1992, and responded to reinstitution of M/P at both relapses. 11. Percentage of CD19+ PBMCs; (W) mlg in serum (g/L); l*)CD19+ cells/ L of blood. 9). This cyclical pattern, with a trough occurring at the end of chemotherapy, was seen for 14 of 19 patients who were analyzed at multiple time points for more than 8 months. For 3 of 19 patients, the percentage of CD38hiB cells remained at a high level throughout the period of analysis, and 2 of 19 showed reduced proportions of CD38hiB cells with the initiation of chemotherapy, which at the time of writing had not yet shown an upswing. DISCUSSION For all patients having a monoclonal band among their BM plasma cells, this study demonstrates the persistent presence of monoclonal CD19' B cells in the blood that share clonotypic VDJ Ig heavy chain rearrangements with the BM plasma cells, as measured by hemi-nested IgH fingerprint analysis, nested CDR3-PCR probedwithanASO, allele- % of CD19+ PBMC I"" expressins CD38 hi I 0' 0 I 1 2 3 4 5 6 7 8 9 1 I 0 Time in months Fig 9. Cyclical expression of high-density CD38 over the course of disease. The expression of CD38"' on large B cells was plotted as a funchon of time postdiagnosis (patients no. 1and 41 or postautolo1: initial time point, gous transplant (patient no.3).Patientno. MGUS; month 6, end of VAD; month 11, pre-autologous BM transplant sample (ABMT). The times are as for Fig 8. Patient no.3: initial time point, post-ABMT; month 6, post-allogeneicBMtransplant; month 14, death. Patient no. 4 initial timepoint, unt; month 6, end of VAD; month 8, Ieukapheresis sample and autologous transplantation. The kinetics of disease for this patient have been presented elsewhere."' Breaks inserted in lines indicate periods longer than l month. Patient no. 1: break, 2 years including a transition from a 2: break,10 diagnosisofMGUS to that of myeloma. Patient no. (B);patient months. Patient no.1is also shown in Fig 8. Patient no.l, no. 2, (+l; patient no. 4 l*). From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 446 Although mean values indicated little change in the circulating B-cell component of myeloma, the values inindividual patients exhibited a wide spread, with normal numbers in some patients. To determine if quantitative normality indicated qualitative normality, physical and phenotypic properties of the B cells were compared. By both measures, the B cells in myeloma blood from untreated and treated patients were highly abnormal, expressing a variety of markers not found on normal resting B cells, including CD38 and CD56. Large CD19+20+38+56+B cells are not found in normal blood. Treatment had no detectable effect on the large Bcell subset. Significant decreases in the number of small €? cells were detectable in patients treated with M/P or VAD. Because small B cells frequently have heterogeneous VDJ Ig rearrangements, this is being evaluated more closely to determine the effects of chemotherapy on the clonotypic subset of small B cells. Extensive DNA aneuploidy comparable to that of BM plasma cells (Pilarski et al, manuscript in preparation) among the small B cells suggests that a large proportion are likely to be within the malignant lineage after ~hemotherapy.'~.'~ The number of small B cells returned to the untreated values once therapy was discontinued. The extensive phenotypic abnormality confirms that, if any normal polyclonal B cells remain in myeloma b l ~ o d , ~they ~.'~ have been altered by the disease process. The CD19+ subsets described here can plausibly be interpreted to represent sequential stages in the malignant B lineage leading to end-stage plasma cells.'o.'6.28The temporal analysis of CD19+ PBMCs in myeloma suggests that chemotherapy does impinge on the circulating CD19+ population, although it does not eradicate clonotypic B cells. Evenin patients with normal numbers, the CD19' PBMCs were phenotypically abnormal, expressing a high density of CD38 and a moderate to high density of CD56. Bothof these markers have been used tocharacterize BM-localized plasma cell^,"^^^ and their appearance on B cells before the acquisition of plasma cell morphology appears to be a late event in B-cell development.i",25,35 Among the blood B cells, the majority of blood B cells withDNA hyperdiploidy were CD38h' (Pilarski et a l l 6 and manuscript in preparation). The lineage relationship betweenBM plasma cells and the clonotypic B cells detected among the CD19+ PBMCs is unknown. Because myeloma is likely to originate from malignant transformation within a chronically stimulated antigen responsive B-cell clone(s), perhaps exemplifiedin monoclonal gammopathies of undetermined significance (MGUS), they could include activated members of the original antigen-responsive clone coexisting with its malignant relatives. Secondly, they could be migratory progeny of a BM-localized or extramedullary stem cell, consistent with their motile phenotype and repertoire of receptors associated with migratory behavior. Finally, they may include the generative stem cell that perpetuates myeloma. Given the heterogeneity of the CD19+ PBMCs and the distribution of clonotypic cells among several CD19+ subsets'" (Bergsagel et al, manuscript in preparation), all of the above interpretations are possible and should not be viewed as mutually exclusive. The results presented here support the notion that the malig- BERGSAGELET AL nant clone in myeloma is heterogeneous, involving multiple differentiation stages with different circulating B-lineage subsets in ascendency at different times and stages of disease. The possibility also exists that similar CD19+ subsets in patients with MGUSi2may reflect dormant myeloma, which, when released from the mechanisms maintaining dormancy, results in the diagnosis of frank myeloma. Overall, the presence of clonotypic cells among CD19+ populations in blood, at times when the BM plasma cells have beenrendered undetectable by chemotherapy, is consistent with properties expected for a drug-resistant reservoir of malignant disease.I5.lb If drug-resistant circulating CD19' cells are responsible for perpetuating myeloma despite killing of the BM-localized plasma cells, new modes of therapy maybe required to eradicate the malignant clone. ACKNOWLEDGMENT This work would not have been possible without the skilled technical assistance of Darlene Paine, Eva Pruski, Dorota Rutkowski, and Kimberly Howland. Joanne Hewitt assisted in collection of clinical information and data entry. Dr Ben Ruether provided some of the patient samples. REFERENCES 1. Dune BGM, Salmon SS: Staging, kinetics, and flow cytometry of multiple myeloma, in Wiemik P, Canellos G, Kyle R, Schiffer C (eds): Neoplastic Diseases ofthe Blood, v01 2. New York, NY, Churchill Livingston, 1985, p 513 2. Greipp PR: Advances in the diagnosis and management of myeloma. Semin Hematol 29:24, 1992 3. Bergsagel DE: Treatment of plasma cell myeloma. Annu Rev Med 30:431, 1979 4. Palmer M, Belch A, Hanson J, Brox L: Reassessment of the relationship between M-protein decrement and survival in multiple myeloma. Br J Cancer 59:l IO, 1989 5. Belch A, Shelley W, Bergsagel D, Wilson K, Klimo P, Willan A: A randomized trial of maintenance versus no maintenance melphalan and prednisone in responding myeloma patients. Br J Cancer 57:94, 1988 6. Jagannath S, Barlogie B, Dicke K, Alexanian R,&gars G, Cheson B, Lemaistre FC, Smallwood L, Pruitt K, Dixon DO:Autologous bone marrow transplantation in multiple myeloma: Identification of prognostic factors. Blood 76:1860, 1990 7. Browman GP, Belch A, Skillings J, Wilson K, Bersagel D, Johnston D, Pater JL: Modified adriamycin-vincristine-dexamethasone (m-VAD) in primary refractory and relapsed plasma cell myeloma: An NCI (Canada) pilot study. 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Smith SH, Brown MH, Rowe D, Callard RE, Beverly PC: Functional subsets of human helper-inducer cells defined by a new monoclonal antibody, UCHLI. Immunology 58:63, 1986 31. Anderson KC, Park EK, Bates MP, Hardy R, Schlossman SF, Nadler LM: Antigens on human plasma cells identified by monoclonal antibodies. J Immunol 130:1132, 1983 32. MacKenzie MR. Paglieroni T, Caggiano V: CD5 positive immunoregulatory B cells in spleen populations from multiple myeloma patients. Am J Hematol 37: 163, 1991 33. Tedder TF, Issacs CM: Isolation of cDNAs encoding the CD19 antigen of human and mouse B lymphocytes. J Immunol 143:712, 1989 34. Zhou L-J, Ord DC, Omori SA, Tedder TF: Structure of the genes encoding the CD19 antigen of human and mouse B lymphocytes. Immunogenetics 35: 102, 1992 35. Tedder TF, Clement LT, Cooper MD: Discontinous expression of a membrane antigen (HB-7) during B lymphocyte differentiation. Tissue Antigens 24:140, 1984 36. Pilarski LM, Mant MJ, Ruether BA, Belch A: Severe deficiency of B lymphocytes in peripheral blood from multiple myeloma patients. J Clin Invest 74:1301, 1984 37. Pilarski LM, Ruether BA, Mant MJ: Abnormal function of B lymphocytes from peripheral blood of multiple myeloma patients. I. Lack of correlation between the number of cells potentially able to secrete IgM and serum IgM levels. J Clin Invest 75:2024, 1985 38. Pilarski LM, Mant MJ, Ruether BA: Review: Analysis of immunodeficiency in multiple myeloma: Observations and hypothesis. J Clin Lab Anal 1:214, 1987 39. van Camp B, Durie BGM, Spier C, de Waele MC, van Riet I, Vela E, Frutiger Y, Richter L, Grogan TM: Plasma cells in multiple myeloma express a natural killer cell-associated antigen: CD56 (NHK-I; Leu-19). Blood 76:377, 1990 From www.bloodjournal.org by guest on February 6, 2015. For personal use only. 1995 85: 436-447 In multiple myeloma, clonotypic B lymphocytes are detectable among CD19+ peripheral blood cells expressing CD38, CD56, and monotypic Ig light chain [published erratum appears in Blood 1995 Jun 1;85(11):3365] PL Bergsagel, AM Smith, A Szczepek, MJ Mant, AR Belch and LM Pilarski Updated information and services can be found at: http://www.bloodjournal.org/content/85/2/436.full.html Articles on similar topics can be found in the following Blood collections Information about reproducing this article in parts or in its entirety may be found online at: http://www.bloodjournal.org/site/misc/rights.xhtml#repub_requests Information about ordering reprints may be found online at: http://www.bloodjournal.org/site/misc/rights.xhtml#reprints Information about subscriptions and ASH membership may be found online at: http://www.bloodjournal.org/site/subscriptions/index.xhtml Blood (print ISSN 0006-4971, online ISSN 1528-0020), is published weekly by the American Society of Hematology, 2021 L St, NW, Suite 900, Washington DC 20036. 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