Gene expression profiling of peripheral blood cells: new insights into Ewing sarcoma biology and clinical applications

Abstract

Ewing sarcoma (ES) is a group of highly aggressive small round cell tumors of bone or soft tissue with high metastatic potential and low cure rate. ES tumors are associated with a rapid osteolysis and necrosis. The currently accepted clinical prognostic parameters do not accurately predict survival of high-risk patients. Moreover, neither the subtype of EWS–FLI1/ERG in the tumor, nor the detection of fusion transcripts in the peripheral blood (PB) samples, has prognostic value in ES patients. We evaluated the prevalence of circulating tumor cells (CTCs) in 34 adult ES patients. Since CTCs were confirmed in only small subset of patients, we further explored the expression profiles of PB leukocytes using a panel of genes associated with immune system status and increased tumor invasiveness. Moreover, we analyzed the alterations of the routine blood tests in the examined cohort of patients and correlated our findings with the clinical outcome. A uniform decrease in ZAP70 expression in PB cells among all ES patients, as compared to healthy individuals, was observed. Monocytosis and the abnormal expression of CDH2 and CDT2 genes in the PB cells significantly correlated with poor prognosis in ES patients. Our study supports the previously proposed hypothesis of systemic nature of ES. Based on the PB cell expression profiles, we propose a mechanism by which immune system may be involved in intensification of osteoclastogenesis and disease progression in ES patients. Moreover, we demonstrate the prognostic value of molecular PB testing at the time of routine histopathological diagnosis.

Introduction

Ewing sarcoma (ES) family of tumors (morphology code: 9260/3 according to the World Health Organization classification of bone tumors) is a group of highly aggressive small round cell tumors of bone and soft tissues, which occur predominantly in adolescents and young adults [1]. ES entity comprises a few types of tumors: Ewing sarcoma of bones, extraskeletal Ewing tumors, primitive neuroectodermal tumors (PNETs), and Askin tumors, which are actually PNETs of the chest wall [1]. Approximately 25 % of patients present with metastatic disease, which is the most prominent adverse prognostic factor [2]. ES metastasizes predominantly via blood, and the most common sites of metastases include lungs, bones, and bone marrow [2]. Roughly half of the patients with localized disease at diagnosis will relapse within 5 years or later after completing the extensive multimodal therapy [3]. Based on the aggressive clinical course and relatively low curative rate, it has been proposed that ES may be a systemic disease characterized by micrometastases at submicroscopic level [4–7].

Manifestation of systemic disorders frequently includes hematologic abnormalities, such as shift in certain blood cell populations and constitutional inflammation. The initial clinical symptoms of ES may include pain, intermittent fever, anemia, increased white blood cell counts, high C-reactive protein concentration, and sedimentation rate, which are the symptoms of systemic inflammatory reactions [1, 8]. ES tumors are also associated with necrosis and rapid, extensive osteolysis [9, 10]. Osteoclast formation in ES is mediated by RANKL-dependent pathway and promoted by the tumor-associated macrophages (TAMs) [8, 9, 11]. TAMs may foster local invasion and are considered as one of the key regulators of cancer-associated inflammation [12]. Macrophage infiltration is an adverse prognostic factor in ES and in many other tumor subtypes including bladder, breast, cervical, and prostate cancers [8]. Also, tumor necrosis facilitates neoplastic progression and has a pro-inflammatory potential [12].

ES tumors are characterized by oncogenic chromosomal translocations detected in 85–95 % of cases. The most common are predominantly balanced t(11;22)(q24;q12) and t(21;22)(q22;q12) translocations, resulting in EWS–FLI1 and EWS–ERG fusion gene formation, respectively [13, 14]. EWS gene (also known as EWSR1—Ewing sarcoma breakpoint region 1) encodes a multifunctional protein involved in DNA-dependent regulation of transcription. FLI1 (Friend leukemia virus integration 1, also known as EWSR2) and ERG [v-ets erythroblastosis virus E26 oncogene homolog (avian)] are closely related members of the erythroblast transformation-specific (ETS) family of transcription factors, containing ETS-type DNA-binding domain [15, 16]. The oncogenic fusion proteins preserve the N-terminal EWS domain and ETS domain of FLI1 or ERG, and function as an aberrant transcriptional activator [14, 17, 18]. In the most prevalent fusion variants, EWS exon 7 is fused to FLI1 exon 6 (type 1), FLI1 exon 5 (type 2), or ERG exon 9 [14, 15]. However, it has been well documented that multiple splice variants of EWS–FLI1 fusion genes may be co-expressed within the same ES tumor [15, 17, 19].

Detection of EWS rearrangements by RT-PCR and/or fluorescence in situ hybridization (FISH) in formalin-fixed paraffin-embedded tissue specimens has become a routine practice in molecular diagnosis of ES [20–22]. Nevertheless, it has been agreed that the fusion subtype does not affect prognosis [23–25]. There are several immunohistochemical markers useful in ES diagnosis, but none of them is exclusively ES-specific. CD99 (encoded by MIC2 gene) is expressed in virtually all cases in a characteristic membranous pattern [26]. Vimentin is also expressed in a large subset of ES tumors [2, 27]. More differentiated ES tumors, especially PNETs, are immunopositive for neural markers such as neuron-specific enolase (NSE) or S-100 protein [2, 28]. Molecular and histological diagnosis of ES is based on tissue specimen obtained with a core or open biopsy, but examination of such material may be hampered by several factors associated with poor representativeness or inadequate fixation method. Biopsy is an invasive procedure that may be accompanied by technical problems due to difficult tumor location or bone sclerosis. Biopsy may also cause discomfort suffered by the patient and subsequent surgical complications. To overcome tumor sampling limitations, sensitive techniques for “liquid biopsy” analysis to monitor cancer genetics in blood have been extensively developed in the recent years [29, 30]. Blood-based molecular biomarkers are likely to be clinically useful, especially for early diagnosis, prognosis, and selection of specific personalized therapy [30]. Several groups have already shown that circulating tumor cells (CTCs) carrying EWS–FLI1/ERG fusion transcripts may be detected in 6–43 % of the peripheral blood (PB) specimens of ES patients at the time of diagnosis but the prognostic significance of these findings remains disputable [4, 5, 31–35]. It has also been demonstrated that gene expression profiling of peripheral blood mononuclear cells (PBMCs) may identify specific functional abnormalities associated with disease outcome and response to therapy in patients with solid tumors [36–42]. Numerous immunological tumor–host interactions involve certain subsets of PBMCs; thus, their gene expression profiles may provide a comprehensive picture of patient’s immune status.

Since the expression of specific fusion genes lacks prognostic significance in ES, microarray technology has been applied to identify prognostically relevant secondary genetic alterations. As a result, numerous genes and pathways associated with the aggressive course of disease have been recognized, including Wnt-signaling, TP53, PI3 kinase pathways, as well as genes involved in cell adhesion, regulation of transcription, and cell cycle control [43–46]. Specifically, the overexpression of CDH11 and MTA1, and down-regulation of CDH2 have been observed in ES patients with poor prognosis [43]. Elevated CCND1 and STEAP1 expression in tumor and bone marrow specimens has been found to correlate with worse patients’ survival [44]. Overexpression of CCND1 has also been detected in primary tumors of ES patients at high risk of metastasis development [45]. CDT2 (also known as DTL) overexpression is another recently identified biomarker of adverse prognosis in ES patients, and it was proposed that the ubiquitin ligase inhibitors may serve as therapeutic agents targeting CDT2 activity [46, 47]. The most important functions of the above-mentioned genes are listed in Table 1.

Table 1.

Selected gene-related functions of adverse prognostic markers identified in ES tumors, according to the NCBI AceView database (http://www.ncbi.nlm.nih.gov/IEB/Research/Acembly/index.html)

No	Gene symbol	Gene name	Function
1	CCND1	Cyclin D1	Cyclin-dependent protein kinase regulator activity, protein kinase activity, cell division, regulation of cell cycle
2	CDH2	Cadherin 2, type 1, N-cadherin (neuronal)	Cell adhesion, calcium-dependent cell–cell adhesion, cell migration
3	CDH11	Cadherin 11, type 2, OB-cadherin (osteoblast)	Cell adhesion, skeletal system development
4	CDT2	Denticleless homolog (Drosophila)	Ubiquitin–protein ligase activity (protein mono- and polyubiquitination), regulation of cell cycle (G2/M transition DNA damage checkpoint), DNA replication
5	MTA1	Metastasis associated 1	Transcription factor activity; regulation of transcription, DNA-dependent
6	STEAP1	Six transmembrane epithelial antigen of the prostate 1	Transporter activity, channel activity

Based on the available tumor-derived data, we sought to identify molecular prognostic markers that could be evaluated in the PB specimens, used as so-called liquid biopsies. We aimed to assess whether the presence of EWS–FLI1/ERG fusion transcripts that characterize CTCs in ES patients correlate with disease outcome. We also studied the expression levels of a panel of genes related to immune status such as ZAP70, NFKB1, IL8, and IL2RA, and increased tumor invasiveness such as CDT2, CDH2, and MTA1, in the PB cells of ES patients. Moreover, we analyzed the alterations in routine blood tests of these patients and correlated our findings with the clinical data. Our study provided a new insight into ES biology and identified potential prognostic markers that can be examined in the PB samples drawn from ES patients at the time of diagnosis.

Materials and methods

Ethics statement

PB specimens were collected after written informed consent had been obtained, according to the protocol approved by the Bioethical Committee of the Maria Sklodowska-Curie Memorial Cancer Center and Institute of Oncology (MSCMCCIO), Warsaw, Poland.

The archival frozen tumor samples obtained from KU Leuven and University Hospitals, Belgium, originate from patient care and were requalified for research. The Ethical Committee of KU Leuven and University Hospitals, Belgium, approved the study.

Study population and ES diagnosis

Thirty-four untreated adult patients diagnosed with ES (20 females and 14 males; median age at diagnosis 27 years, range 19–59 years) and 13 healthy individuals (7 females and 6 males, median age 37 years, range 23–68 years) were recruited for this prospective study (Table 2) between July 2008 and October 2011 at the MSCMCCIO.

Table 2.

Clinical, pathological, and molecular features of patients with ES family of tumors

No	Nested RT-PCR in PB	FISH assay	Sex	Age	Primary site	Size of primary tumor (cm)	M0/M1 status at diagnosis	Last follow-up (months/latest status)
1	Neg	Pos	F	24	Iliac bone	>10	M1	33/DOD
2	Neg	NA	M	19	Tibia	10	M0	62/AWOD
3	Neg	NA	F	20	Paraspinal	NA	M1	15/DOD
4	Neg	Pos	M	59	Scapula	6	M0	61/AWOD
5	Neg	NA	F	29	Femur	NA	M0	53/AWOD
6	Neg	Pos	F	29	Ischium	>10	M0	5/DOD
7	Pos (EWS–ERG)	Pos	M	42	Iliac bone	>10	M1	9/DOD
8	Neg	Pos	F	20	Femur	14	M1	7/DOD
9	Neg	Pos	F	25	Iliac bone	>10	M1	55/AWD
10	Neg	Pos	M	33	Femur	7	M0	50/AWOD
11	Neg	NA	M	37	Chest wall	15	M0	49/AWOD
12	Neg	Pos	F	40	Tibia	>10	M0	7/DOD
13	Neg	NA	M	24	Chest wall	>10	M1	4/DOD
14	Neg	NA	F	19	Femur	>10	M0	1/AWD
15	Neg	Pos	F	19	Scapula	9.5	M0	44/AWOD
16	Neg	Pos	M	22	Femur	11	M1	6/DOD
17	Neg	NA	F	33	Forearm	7	M0	43/AWOD
18	Neg	NA	M	20	Humerus	NA	NA	NA/AWD
19	Neg	Pos	M	25	Fibula	10	M0	15/DOD
20	Neg	Pos	M	27	Costa	NA	M0	34/DOD
21	Neg	NA	F	37	Paraspinal	12	M0	14/DOD
22	Neg	NA	F	30	Thigh	8.5	M1	25/DOD
23	Neg	NA	F	30	Femur	NA	M0	37/AWD
24	Neg	NA	F	24	Retroperitoneal space	NA	M0	37/AWD
25	Neg	Pos	F	25	Forearm	9.5	M0	33/AWOD
26	Neg	NA	F	34	Humerus	NA	M0	34/AWD
27	Neg	NA	F	27	Pelvis	NA	M1	14/DOD
28	Neg	Pos	M	41	Abdominal wall	7	M1	34/AWD
29	Pos (EWS–FLI1 type 2)	Pos	F	23	Pelvis	NA	M1	3/DOD
30	Neg	NA	M	43	Femur	NA	M0	10/DOD
31	Neg	NA	M	20	Ribs	17	M0	28/AWOD
32	Neg	Pos	F	29	Mediastinum	15	M0	111/AWD
33	Pos (EWS–FLI1 type 1)	NA	F	21	Ischium	8	M1	18/DOD
34	Neg	NA	M	35	Femur	13	M0	26/AWOD

RT-PCR reverse transcription polymerase chain reaction, FISH fluorescent in situ hybridization, M0 no evidence of metastasis, M1 evidence of metastasis, Pos positive, Neg negative, NA not available, DOD dead of disease, AWD alive with disease, AWOD alive without disease

The diagnosis of ES was established on FFPE tissue specimens using standard pathologic criteria and supported by immunohistochemistry and FISH analysis in the Department of Pathology, MSCMCCIO. FISH analysis for the detection of EWS gene rearrangement using LSI EWSR1 (22q12) dual-color, break-apart rearrangement probe (Abbott Molecular) was performed using standard methods. Tumors with negative or non-informative FISH result were diagnosed as ES based on the combination of morphological and immunohistochemical features, evaluated independently by two pathologists (A.S.C. and K.P.). Differential diagnosis excluded cancer, lymphoma, melanoma, rhabdomyosarcoma, synovial sarcoma, and other sarcoma subtypes in these cases.

Peripheral blood (PB) specimens’ preparation and extraction of total RNA

Approximately 10 ml of PB was drawn into EDTA tubes (250 μl, 0.5 M, pH = 8) before the diagnostic biopsy and the beginning of a multimodal chemotherapy, radiotherapy, and surgery (when possible) according to the established treatment protocols [48]. Each PB specimen was divided into two portions and centrifuged (3000 rpm, 10 min, at room temperature) in order to separate blood cells from plasma. The bottom fraction containing red blood cells and the buffy coat containing leukocytes, platelets, and circulating tumor cells (CTCs) were used to extract total RNA with TRI Reagent BD (Sigma) and subsequent DNase treatment using RNease-free DNase set (Qiagen, Valencia, CA, USA), according to the manufacturers’ protocols. RNA quantity and quality were evaluated using NanoDrop 2000 Spectrophotometer (Thermo Scientific, Waltham, MA, USA) and FlashGel system (Lonza, Basel, Switzerland).

Hematological analysis

Standard hematological parameters were evaluated by laboratory blood tests in ES patients and healthy individuals at the time of diagnosis, as a routine admission procedure at the MSCMCCIO. PB specimens for routine blood tests and for this study were drawn at the same time. We evaluated the following parameters: hemoglobin level (HGB), platelet count (PLT), white blood cell count (WBC), neutrocyte count (NE), lymphocyte count (LY), and monocyte count (MO).

Tumor specimens and ES cell line

Archival frozen tumor specimens and RD-ES cell line served as positive controls for nested RT-PCR experiments. Frozen tumor samples from 5 untreated ES patients were obtained from KU Leuven and University Hospitals, Belgium (4 primary tumors and 1 metastatic tumor; 4 males and 1 female; median age 25 years, range 4–43 years). Total RNA from the frozen tumor specimens was extracted using miRNeasy kit (Qiagen) including DNase treatment using RNease-free DNase set (Qiagen) according to the manufacturer’s protocol. RNA quantity was determined using NanoDrop 2000 Spectrophotometer (Thermo Scientific), and the quality was evaluated using Bio-Rad Experion RNA StdSens Analysis system (Bio-Rad, Hercules, CA, USA). RD-ES cell line carrying EWS–FLI1 type 2 translocation was purchased from CLS Cell Lines Service GmbH. Total RNA was extracted from RD-ES cells using RNeasy kit (Qiagen) according to the manufacturer’s protocol. RNA quantity and quality were evaluated using NanoDrop 2000 Spectrophotometer (Thermo Scientific) and FlashGel system (Lonza), respectively.

Isolation and culture of PBMCs

Peripheral blood mononuclear cells (PBMCs) specimens were obtained from the Department of Immunology, MSCMCCIO. PBMCs of 3 healthy donors were obtained by standard Ficoll-Paque (Pharmacia/Pfizer, New York City, NY, USA) gradient centrifugation. Samples of non-cultured cells were taken, and the remaining cells were cultured in a standard RPMI-1640 medium with l-glutamine (Gibco/Thermo Scientific, Waltham, MA, USA), supplemented with 10 % heat-inactivated FCS (Gibco) and gentamycin (Sigma, 50 μg/ml), for 4 days in the presence of phytohemagglutinin (PHA, Wellcome/GlaxoSmithKline, Brentford, England; 1 μg/ml). Cells were centrifuged, washed twice in PBS, and the cell pellet was kept frozen at −70 °C until RNA was isolated. Total RNA was isolated from PBMCs with the use of RNeasy kit (Qiagen). The quantity and quality of the RNA were examined using NanoDrop 2000 Spectrophotometer (Thermo Scientific) and by denaturing gel electrophoresis with ethidium bromide.

Nested reverse transcription PCR (nested RT-PCR)

Nested RT-PCR was performed to detect EWS–FLI1/ERG fusion transcripts in CTCs and tumor specimens, according to the modified protocol described by Peter et al. [31], which allows detection of 1 tumor cell per million of mononuclear blood cells. One microgram of total RNA was reverse-transcribed with oligo(dT)_12–18 primers and random hexamers using SuperScript II Reverse Transcriptase (Invitrogen/Thermo Scientific, Waltham, MA, USA). cDNA quality was assessed by PCR using GAPDH primers (Table 3).

Table 3.

Primers used for RT-PCR, nested RT-PCR, and direct sequencing

Designation	Sequence	Direction	NCBI reference sequence
GAPDH1	5′ GGTCGGAGTCAACGGATTTG 3′	Forward	NM_002046.4
GAPDH2	5′ ATGAGCCCCAGCCTTCTCCAT 3′	Reverse	NM_002046.4
22.8	5′ CCCACTAGTTACCCACCCCAAA 3′	Forward	NM_013986.3
22.3	5′ TCCTACAGCCAAGCTCCAAGTC 3′	Forward	NM_013986.3
FLI11	5′ AGGGTTGGCTAGGCGACTGCT 3′	Reverse	NM_002017.4
FLI3	5′ GTCGGGCCCAGGATCTGATAC 3′	Reverse	NM_002017.4
ERG11	5′ TGTTGGGTTTGCTCTTCCGCTC 3′	Reverse	NM_182918.3
ERG3	5′ ACTCCCCGTTGGTGCCTTCC 3′	Reverse	NM_182918.3

EWS–FLI1 and EWS–ERG fusion junctions were detected using AmpliTaq Gold DNA Polymerase (Invitrogen). The first round of amplification was performed with 2.5 μl of cDNA using primers appropriate for EWS and FLI1/ERG genes (22.8 and FLI11/ERG11, respectively), and the second round of amplification was performed using one-fifth of the first round PCR product, with internal primers appropriate for EWS and FLI1/ERG genes (22.3 and FLI3/ERG3, respectively) (Table 3). The first and second round of amplifications were performed in 25 μl volumes at 94 °C for 30 s, 68 °C for 60 s, and 72 °C for 60 s for 15 and 35 cycles, respectively, and the final extension was performed for 10 min in both reactions. cDNA from RD-ES cell line and frozen tumor specimens were used as positive controls. Appropriate negative controls were also included in every step of the procedure. PCR products were visualized by electrophoresis in 2 % TBE agarose gels stained with ethidium bromide, purified using ExoSAP-IT, PCR Product Clean-Up (Affymetrix, Santa Clara, CA, USA) and prepared for direct sequencing using BigDye^® Terminator version 3.1 Cycle Sequencing Kit (Life Technologies) with subsequent precipitation using ExTerminator kit (A&A Biotechnology, Gdynia, Poland). Samples were analyzed using the 3130×L Genetic Analyzer (Life Technologies).

Quantitative reverse transcription PCR (qRT-PCR)

Five hundred nanogram of total RNA was reverse-transcribed with oligo(dT)_12–18 primers and random hexamers using High-Capacity cDNA Reverse Transcription kit (Life Technologies). cDNA quality was assessed by PCR using GAPDH primers (Table 3). All reactions were performed in duplicate or triplicate using the TaqMan Gene Expression Assays (Life Technologies) (Table 4) in the 7500 Fast Real-Time PCR System (Life Technologies), according to the manufacturer’s recommendations. Experimental data were analyzed using threshold-cycle (Ct) values generated in the SDS 2.1 software (Life Technologies). Mean expression level of two reference genes PSMC4 and EIF2B1 served as endogenous control. Endogenous controls were selected from a set of 4 candidate genes (EIF2B1, MRPL19, POP4, and PSMC4) based on the most stable expression across different sample types (blood, tumor tissue, and cell line), which was calculated using geNorm [49] and NormFinder [50] algorithms. Negative controls were also included in every step of the procedure. Total RNA from RD-ES cell line served as an inter-plate calibrator.

Table 4.

TaqMan assays (Applied Biosystems) used in qRT-PCR experiments

Gene symbol	Assay category	Assay ID
PSMC4	Control assay	Hs00197826_m1
EIF2B1	Control assay	Hs00426752_m1
CCND1	Gene expression assay	Hs00765553_m1
CDH1	Gene expression assay	Hs01023894_m1
CDH2	Gene expression assay	Hs00983056_m1
CDH11	Gene expression assay	Hs00901475_m1
CDT2	Gene expression assay	Hs00978565_m1
MTA1	Gene expression assay	Hs00950776_m1
STEAP1	Gene expression assay	Hs00185180_m1
IL8	Gene expression assay	Hs00174103_m1
IL2RA	Gene expression assay	Hs00907779_m1
NFKB1	Gene expression assay	Hs00765730_m1
ZAP70	Gene expression assay	Hs00896347_m1

Data analysis

Chromas Lite 2.01 software (Technelysium Pty, Ltd, South Brisbane, Australia) and BLAST software were used for the analysis of sequencing data (http://blast.ncbi.nlm.nih.gov/Blast.cgi).

Relative gene expression levels were calculated using 2^−ΔΔCt method [51]. Statistical analysis was performed using GraphPad QuickCalcs (Grubbs’ test to detect outliers; t test to compare two means between groups; chi-square test for contingency tables analysis) (GraphPad Software, Inc., La Jolla, CA, USA).

For the survival analysis, the Kaplan–Meier estimator was used with the log-rank tests for bivariate comparisons using STATISTICA 7.0 software (Statsoft, Tulsa, OK, USA). Overall survival (OS) time for the assessment of prognostic value of clinical and molecular parameters was calculated from the date of start of therapy to the date of the most recent follow-up (censored data) or death. The differences were considered statistically significant if the p values were below 0.05.

Results

Detection of EWS–FLI1/ERG fusion transcripts

Total RNA and cDNA were obtained from PB specimens of all 34 patients. CTCs carrying typical EWS–FLI1 and EWS–ERG transcripts were detected in 19 % (n = 3) of patients with positive FISH result in FFPE tumor specimen. Typical type 1 or 2 EWS–FLI1 transcripts were detected in all five frozen tumor specimens and RD-ES cell line used as controls. Specificity of nested RT-PCR blood tests for both EWS–FLI1 and EWS–ERG detection was 100 % (95 % CI 73.35 to 100.0 %).

In 76 % (n = 26) of ES patients, the unexpected, shorter EWS–FLI1 transcripts were detected; however, these transcripts were not detectable when 10× dilution of the first round PCR product was used for nested amplification (Fig. 1). Nevertheless, the sequence analysis revealed that these unusual rearrangements cause a shift of the reading frame, resulting in the introduction of premature STOP codons. The predicted truncated chimeric proteins do not preserve any functional domains of FLI1 protein, and therefore, most likely are not oncogenic.

Fig. 1.

Nested RT-PCR products obtained from the control frozen tumor tissues and PB specimens of ES patients visualized by electrophoresis in 2 % agarose gel stained with ethidium bromide. a The second round of amplification was performed using one-fifth of the first round PCR product. b The second round of amplification was performed using one-fifth of the 10× dilution of the first round PCR product. M: 1-kb Plus DNA ladder (Invitrogen). Lanes 1–5 PCR products from frozen tumor tissues; lanes 6–11 PCR products from selected PB specimens from ES patients; lanes 12, 13 PCR negative controls for two rounds of amplification; lane 14 positive control, EWS–FLI1 type 2 fusion (RD-ES cell line). Lanes 2, 3, 5, and 10 EWS–FLI1 type 1 fusions, lanes 1 and 4 EWS–FLI1 type 2 fusions

Hematological abnormalities in ES patients

Results of the laboratory blood tests were available for 33 ES patients and 10 healthy individuals. One or more parameters outside the reference range were found in 85 % (n = 29) of ES patients. The most frequent blood test alterations in ES patients were decreased HGB level (67 %; n = 22), monocytosis (36 %; n = 12), lymphocytopenia (36 %; n = 12), thrombocytosis (27 %; n = 9) and neutrophilia (27 %; n = 9), and increased WBC count (21 %; n = 7). Anemia, as defined by WHO criteria [52], was observed in 52 % (n = 17) of ES patients at the enrollment. Hematological data for ES patients and healthy individuals are summarized in Tables 5 and 6.

Table 5.

Results of standard hematological tests in ES patients

	WBC (× 109/l)	HGB (g/dl)	PLT (× 109/l)	NE (× 109/l)	LY (× 109/l)	MO (× 109/l)
Mean ± SD	8.07 ± 3.76	11.98 ± 1.66	334.7 ± 103.64	5.4 ± 3.01	1.8 ± 0.82	0.83 ± 0.51
Above the reference upper limit
n	7	0	9	9	2	12
%	21	0	27	27	6	36
Below the reference lower limit
n	3	22	1	6	12	1
%	9	67	3	18	36	3

WBC white blood cell count, HGB hemoglobin level, PLT platelet count, NE neutrocyte count, LY lymphocyte count, MO monocyte count, l liter, g/dl gram per deciliter, SD standard deviation

Table 6.

Results of standard hematological tests in healthy individuals

	WBC (×109/l)	HGB (g/dl)	PLT (×109/l)	NE (×109/l)	LY (×109/l)	MO (×109/l)
Mean ± SD	9.32 ± 5.67	13.66 ± 1.37	252.10 ± 83.17	6.36 ± 4.79	2.05 ± 0.77	0.64 ± 0.41
Above the reference upper limit
n	1	0	1	2	2	1
%	10	0	10	20	20	10
Below the reference lower limit
n	0	3	0	0	2	0
%	0	30	0	0	20	0

WBC white blood cell count, HGB hemoglobin level, PLT platelet count, NE neutrocyte count, LY lymphocyte count, MO monocyte count, SD standard deviation

Gene expression results

cDNA from 23 ES patients, 9 healthy individuals, and RD-ES cell line was available for quantitative gene expression experiments. We observed significant down-regulation of ZAP70 expression in all ES patients as compared to healthy controls (p < 0.0001) (Fig. 2a). Also, CDH2 was significantly down-regulated in the majority of ES patients (p = 0.0083) (Fig. 2b), with more than twofold decrease in the relative CDH2 expression level in PB cells observed in 14 ES patients. Moreover, CDT2 and IL8 were significantly overexpressed, each in 4 ES patients (p < 0.0001 and p = 0.0047, respectively). The upper limit of normal CDT2 and IL8 expression level was defined as mean expression level +2 standard deviations (SD) in healthy controls.

Fig. 2.

Analyses of the relative gene expression level of a ZAP70 and b CDH2 genes performed by qRT-PCR, using RNA samples from PB cells of ES patients and healthy individuals. The error bars represent standard deviation from the mean 2^−ΔΔCt

Expression of STEAP1 and CDH11 could not be detected in any of the PB specimens. No significant differences between ES and control PB specimens were observed regarding CCND1, CDH1, MTA1, IL2RA, and NFKB1 expression.

Mitogen-activated lymphocytes were characterized by significant down-regulation of ZAP70 expression (p = 0.017), and overexpression of CDT2 (p = 0.008), as compared to the unstimulated PBMCs.

Correlation of hematological and genetic findings in PB with the clinical outcome

The median follow-up for all 34 ES patients involved in this study was 28 months (range 1–111 months). At the time of last follow-up, 30 patients completed the treatment procedure, two patients continued therapies in other centers, in two cases the therapy was interrupted because of patient’s death. During the follow-up period, 16 patients died from disease and another 3 patients had documented progression of the disease.

All three patients with confirmed CTCs had distant metastases at the time of diagnosis and died from ES during follow-up.

The Kaplan–Meier analysis demonstrated significantly worse OS in patients with at least twofold CDH2 down-regulation and CDT2 overexpression in PB cells at the time of enrollment (p = 0.01 and p = 0.02, respectively) (Figs. 3a, b). Also, monocytosis correlated with significantly shorter OS in ES patients (p = 0.02) (Fig. 3C). IL8 overexpression did not affect the probability of survival (p = 0.3).

Fig. 3.

Kaplan–Meier analysis of overall survival (OS) according to a at least twofold decrease in CDH2 expression level and b CDT2 overexpression and c monocytosis in PB specimens

Discussion

We demonstrated the presence of CTCs carrying oncogenic EWS–FLI1/ERG fusions in only 19 % (n = 3) of ES patients with confirmed EWS/FLI1 rearrangements in tumor specimen. Roughly comparable chimeric transcript detection rates in PB specimens of ES patients at diagnosis have been also reported in previously published series [31, 34, 35]. Detection of CTCs in only small subset of patients prompted us to investigate hematological profiles and expression levels of genes related to immune status and increased tumor invasiveness in PB specimens of ES patients. We selected CCND1, MTA1, STEAP1, CDH2, CDH11, and CDT2 genes that are known to be involved in metastatic spread in several sarcoma subtypes, and their abnormal expression in tumors correlates specifically with poor prognosis in ES patients [43–46]. We also examined the expression level of CDH1 gene, encoding E-cadherin, which mediates the formation of chemoresistant spheroids from non-adherent ES cells by the activation of the ERBB4 tyrosine kinase, induction of the PI3K-AKT pathway, and suppression of anoikis [53]. In addition, we chose four genes that would provide an insight into different aspects of immune status of ES patients. ZAP70 encodes cytoplasmic tyrosine kinase, which plays a central role in the initiation of T-cell response [54]. NFKB1 codes for a DNA-binding subunit of the NF-kappa-B (NFκB) protein complex transcription regulator, and altered expression of this gene is associated with cancer and many inflammatory diseases [55]. Interleukin 8 (IL-8) is a pro-inflammatory chemokine that promotes angiogenesis, tumor progression, invasion, and metastasis [56]. IL-8 is expressed in monocytes and macrophages, and both macrophage infiltration and high expression level of IL8 correlate with poor outcome in ES patients [8, 57]. IL2RA encodes a soluble subunit of IL-2 receptor expressed on activated lymphocytes [58].

We observed a uniform decrease in ZAP70 expression among all ES patients compared to healthy individuals. An impaired expression of ZAP70 and/or associated zeta chain protein was previously described in activated circulating T cells, and connected with poor prognosis of patients with head and neck, lung, laryngeal squamous cell carcinoma, and melanoma [59–62]. ZAP70 is rapidly degraded in antigen-activated T lymphocytes, in parallel with zeta chain and T-cell receptors (TCRs) [63]. Also, in our specimens of normal mitogen-activated T lymphocytes, ZAP70 was significantly down-regulated as compared to unstimulated PBMCs. Moreover, the lack of NFKB1 activation in the circulating leukocytes of the examined ES patients argues for the inactivation of ZAP70 signaling pathway. We suggest that decreased expression of ZAP70 may reflect a sustained activation of circulating T cells. This assumption goes in line with the previous evidence of circulating tumor-reactive T lymphocytes in ES patients [64]. Moreover, elevated CDT2 expression level in PB in a subset of ES patients may be linked with the presence of activated circulating T lymphocytes. Our results in normal PBMCs, just like the data retrieved from the Genevestigator database (www.genevestigator.com/gv/biomed.jsp) [65], showed CDT2 overexpression following stimulation. We propose that there may be an apparent interplay between activated T lymphocytes and ES cells, since both can trigger RANKL-mediated osteoclastogenesis [9, 66, 67]. Osteoclasts differentiate from the proliferative monocyte fraction of PBMCs and from TAMs [11, 68]. Also, TAMs themselves derive from the circulating monocytes that are selectively attracted to the tumor microenvironment [69]. We speculate that there may be a mechanism linking the aggressive course of ES and T-cell activation, intensified osteoclast formation, bone lysis, and necrosis. In our study, in over one-third of patients, we demonstrated monocytosis, which significantly correlated with worse disease outcome. Moreover, we observed worse OS in patients with a strong decrease in CDH2 expression in PB cells, and CDH2 down-regulation is a characteristic feature of osteoclasts and their precursors [70, 71]. There was a significant correlation between monocyte count and CDH2 expression level in our study (p = 0.04), and we noted at least twofold CDH2 down-regulation in all but one of the patients with monocytosis. Interestingly, monocytosis is frequently induced by necrosis [72], and TAMs tend to accumulate into necrotic regions of tumors [69]. This interpretation further supports the notion that ES is a systemic disease; however, to verify this concept, elaborate functional studies are necessary.

Our study shows that adult ES patients present specific hematological abnormalities. Alterations in routine blood tests have previously been examined in soft tissue sarcoma patients; however, correlations of these parameters with particular histological subtypes have not been examined [73]. In our cohort of ES patients, hematological disturbances were observed in 85 % of cases, which is twice as much than Ruka et al. [73] have shown in other sarcoma subtypes. Most prevalent hematological alterations observed across diverse sarcoma subtypes were neutrophilia, leucocytosis, decreased HGB level, monocytosis, and thrombocytosis, in descending order [73]. In ES patients, frequencies of blood test abnormalities were different, with decreased HGB level being the most frequent, followed by monocytosis, lymphocytopenia, thrombocytosis, neutrophilia, and increased WBC count. These abnormalities did not correlate with clinicopathological features, such as metastatic status or tumor size at diagnosis. Considering the increased monocyte count and the above-described molecular findings, there is a possibility that the proliferative fraction of circulating monocytes plays a significant role in ES biology.

The most important clinical implication of our findings is a considerable CDH2 down-regulation in PB specimens of patients with worse OS. Decrease in CDH2 expression has previously been correlated with poor prognosis in ES, rhabdomyosarcoma, and Wilms’ tumors [43]. It has also been demonstrated that both CDH2 and N-cadherin down-regulations dramatically change glioma cells migratory behavior and increases invasiveness of this non-epithelial tumor [74]. Based on the results presented here, we postulate that the combination of disseminated disease (M1) at diagnosis, which is a well-established clinical prognostic factor in ES, with molecular evaluation of CDH2 expression may be a better predictor of poor prognosis in ES patients than the metastatic status alone. Such combination clearly distinguished between patients who died of disease and were alive at the last follow-up time point (Fig. 4). Detection of symptoms of systemic disease in ES patients may change the current prognostic scoring model and influence therapeutic decisions. Based on the unfavorable results of hematological and molecular examination of PB specimens, patients with macroscopically localized disease may be qualified for more aggressive treatment, so far dedicated to patients with disseminated disease, such as chemotherapy intensified either by dose escalation, or by the addition of new agents. High-dose chemotherapy with autologous hematopoietic stem cell rescue may also be considered in these patients. Prognostic implications of PB testing in ES patients warrant further studies.

Fig. 4.

Kaplan–Meier analysis of overall survival (OS) according to a M0/M1 status at diagnosis, and b M1 at diagnosis combined with at twofold decrease in CDH2 expression level

To conclude, our study supports the hypothesis of systemic nature of ES. We show evidence of immune involvement in ES and point to the possible mechanism by which immune system may be involved in osteoclastogenesis intensification and progression in ES. Furthermore, we demonstrate the significant prognostic power of CDH2 expression in PB cells in terms of OS, especially when combined with metastatic status at the time of routine pathologic diagnosis.