Tissue factor-dependent and -independent pathways of systemic coagulation activation in acute myeloid leukemia: a single-center cohort study
- Christina Dicke†1,
- Ali Amirkhosravi†2,
- Brigitte Spath1,
- Miguel Jiménez-Alcázar3,
- Tobias Fuchs3,
- Monica Davila2,
- John L Francis2,
- Carsten Bokemeyer1 and
- Florian Langer1Email author
© Dicke et al. 2015
Received: 23 June 2015
Accepted: 29 July 2015
Published: 6 August 2015
In acute myeloid leukemia (AML), disseminated intravascular coagulation (DIC) contributes to morbidity and mortality, but the underlying pathomechanisms remain incompletely understood.
We conducted a prospective study on 69 patients with newly diagnosed AML to further define the correlates of systemic coagulation activation in this hematological malignancy. Tissue factor procoagulant activity (TF PCA) of isolated peripheral blood mononuclear cells (PBMCs) and TF expression by circulating microparticles (MPs) were assessed by single-stage clotting and thrombin generation assay, respectively. Soluble plasma TF antigen and secretion of vascular endothelial growth factor (VEGF) by cultured PBMCs were measured by ELISA. Cell-free plasma DNA was quantified by staining with a fluorescent dye.
TF PCA of PBMCs was significantly increased in AML patients as compared to healthy controls. Furthermore, TF PCA was significantly associated with decompensated DIC at presentation, as defined by a plasma fibrinogen level of ≤1 g/L (n = 11). In addition to TF PCA and circulating blasts, serum lactate dehydrogenase, a surrogate marker for leukemic cell turnover, correlated with plasma D-Dimer in the total patient cohort and was significantly increased in DIC patients, suggesting a role for myeloblast apoptosis/necrosis in activation of the TF-dependent coagulation pathway. Consistently, TF-bearing plasma MPs were more frequently detected and levels of soluble TF antigen were significantly higher in DIC vs. non-DIC patients. No association was found between TF PCA expression and VEGF secretion by isolated PBMCs, but significantly increased levels of cell-free plasma DNA pointed to a contribution of the intrinsic contact pathway to systemic coagulation activation in the total patient cohort and in patients with lower TF PCA expression. While PBMC-associated TF PCA had no effect on long-term survival, DIC occurrence at presentation increased the risk of early mortality.
In newly diagnosed AML, TF expression by PBMCs and shedding of TF-bearing plasma MPs are central to the pathogenesis of DIC, but additional pathways, such as DNA liberation, may contribute to systemic coagulation activation.
KeywordsAcute myeloid leukemia Tissue factor Disseminated intravascular coagulation Cell-derived microparticles DNA
Acute myeloid leukemia (AML) is a highly aggressive hematological malignancy characterized by clonal expansion of transformed myeloblasts. Patients with AML are at increased risk for both hemorrhagic and thromboembolic complications [1–3]. Besides disease- or treatment-related thrombocytopenia, AML patients may suffer from complex systemic coagulopathies such as overt disseminated intravascular coagulation (DIC), excessive fibrinolysis, or non-specific proteolysis. In particular, patients with acute promyelocytic leukemia (APL) are at substantial risk for a thrombohemorrhagic syndrome that, despite modern anti-leukemic therapy, still significantly contributes to early morbidity and mortality .
In newly diagnosed AML, potentially large numbers of myeloblasts circulate in direct contact with the plasma compartment. It is thus very likely that the procoagulant (or fibrinolytic) phenotype of AML blasts will have a profound effect on the hemostatic system. In fact, early studies have implicated over-expression of tissue factor (TF), the principal initiator of the extrinsic coagulation protease cascade, in the pathogenesis of AML-associated DIC [5–8]. More recent studies, however, have questioned the relevance of TF-driven coagulation activation to the hypercoagulable state in various hematological malignancies, including AML, and suggested alternative mechanisms such as acquired activated protein C resistance [9, 10].
Because a thorough understanding of the cellular and molecular pathways underlying AML-associated DIC is mandatory to identify novel drug targets for the prevention and treatment of potentially fatal thrombohemorrhagic events, we conducted a prospective study to further define the correlates of systemic coagulation activation in 69 patients with newly diagnosed AML.
Demographic, clinical and laboratory characteristics of AML patients
Patients (n = 69)
59 ± 16
Peripheral blasts (103/µL)
9.6 ± 1.9
Prothrombin time (%)
79 ± 23
4.3 ± 2.3
TF PCA of PBMCs is increased in AML
TF PCA of PBMCs was significantly increased in AML patients (n = 69) as compared to healthy controls (n = 10) (Fig. 1a), suggesting that leukemic transformation was associated with upregulation of the TF-dependent coagulation pathway. However, PBMC-associated TF PCA varied widely among study subjects with 50 AML patients (72%) having TF PCA levels within the reference range, the upper limit of which was defined as the 95th percentile of TF PCA levels of intact PBMCs within the control group. To compare PBMC-associated TF PCA expression in newly diagnosed AML with that in other hematological malignancies, we also studied patients with MDS or acute lymphoblastic leukemia (ALL). There were no statistically significant differences in median TF PCA levels between AML patients (n = 69) and patients with either MDS (n = 7) or ALL (n = 5), albeit none of the latter patients had a PBMC-associated TF PCA level of >1,500 AU/106 cells (Fig. 1a). Collectively, these findings indicate that PBMC-associated TF PCA is overexpressed at least in a subgroup of patients with newly diagnosed AML.
TF PCA expression among FAB subtypes
To analyze PBMC-associated TF PCA expression among subtypes of the French–American–British (FAB) classification, AML patients (n = 69) were grouped in those with M0/M1/M2 (n = 32), M3 (n = 5), M4/M5 (n = 19) or secondary AML (n = 13) (Fig. 1b). When compared to healthy controls, TF PCA levels of both intact and disrupted PBMCs were significantly increased in each of these subgroups [not shown]. When compared among each other, patients with APL (M3) had significantly higher TF PCA levels than patients included in the other subgroups, although values of PBMC-associated TF PCA were overlapping with those in the M0/M1/M2 and M4/M5, but not with those in the secondary AML subgroup (Fig. 1b).
Markers of systemic coagulation activation
Because plasma D-dimer is readily available and widely used in clinical practice and part of the SSC/ISTH DIC score , this parameter was chosen to assess systemic coagulation activation in our study. However, D-dimer originates from plasmin-mediated degradation of cross-linked fibrin and therefore reflects fibrinolytic rather than procoagulant activity. In contrast, circulating thrombin–antithrombin (TAT) complexes are a more accurate marker of in vivo thrombin generation. To investigate the usefulness of D-dimer as a hemostatic activation marker in newly diagnosed AML, we additionally measured circulating TAT complexes in a subgroup of 20 AML patients, the selection of which was based on the degree of D-dimer elevation (low vs. high) and availability of plasma samples. In this subgroup, there was a quite strong correlation between the two parameters (Fig. 1c). Follow-up plasma samples were available from two patients achieving complete hematological remission after the first cycle of induction chemotherapy. Plasma levels of D-dimer and TAT complexes either normalized or decreased close to normal in both patients (Fig. 1d), further indicating that plasma D-dimer may be an appropriate marker of systemic coagulation activation in newly diagnosed AML, particularly in the absence of recent surgery, acute infections, and relevant organ dysfunctions, all of which were exclusion criteria in our study (see section “Methods”).
When analyzing the total AML patient cohort (n = 69), only two patients (3%) had D-dimer plasma levels within the reference range (i.e. <0.5 mg/L). Similar to PBMC-associated TF PCA, plasma D-dimer levels were highest in the M3 subgroup, but levels exceeding 30 mg/L were also observed in the M0/M1/M2 and M4/M5 subgroups (Fig. 1e).
Role of cellular TF PCA in DIC evolution
Characteristics of patients with decompensated DIC at presentation
TF PCA (AU/106 cells)
MP TF PCA
TF antigen (pg/mL)
Deceased after 3 days (fatal PE)
Deceased after 2 days (fatal ICH)
Deceased after 4.3 months
Alive at 69 months follow-up
Deceased after 6 days (fatal ACS)
Alive at 23 months follow-up
Alive at 52 months follow-up
Deceased after 2.9 months (fatal pneumonia)
Deceased after 5 days (fatal ICH)
Deceased after 8.3 months
Deceased after 4.4 months (recurrent AML with DIC)
TF PCA of plasma microparticles is associated with DIC
Cellular TF PCA is not correlated with VEGF secretion
Potential role of cell-free DNA in intravascular coagulation activation
Recently, neutrophil extracellular traps (NETs) have been identified as activators of blood coagulation [17, 18]. Furthermore, NETs are associated with various cancer-associated clotting disorders , including deep-vein thrombosis and thrombotic microangiopathies [20–22]. DNA is a major component of NETs and sufficient to accelerate blood clotting . We therefore asked if increased levels of cell-free DNA could account for systemic coagulation activation, as assessed by plasma D-dimer, in our AML patient cohort. Plasma for DNA quantification was not available from four AML patients, including three patients with DIC. Compared to healthy controls (n = 10), AML patients (n = 65) had significantly increased levels of cell-free plasma DNA (Fig. 5c). In AML patients, extracellular DNA levels significantly correlated with plasma D-dimer (r = 0.31, P = 0.011) and serum LDH (r = 0.37, P = 0.002), but not with peripheral blasts (r = 0.22, P = 0.080). To further explore the relevance of cell-free DNA for systemic coagulation activation, AML patients (n = 65) were grouped into those with plasma DNA levels of >110 ng/mL (n = 43), corresponding to the 95th percentile of plasma DNA levels within the control cohort, and those with plasma DNA levels of ≤110 ng/mL (n = 22). Patients with cell-free DNA levels above this cut-off value had significantly increased plasma D-dimer (Fig. 5d). In a subsequent analysis, we excluded all DIC patients with TF PCA levels of intact PBMCs exceeding 2,500 AU/106 cells (n = 7), because in these patients, expression of TF PCA was considered the predominant cause of systemic coagulation activation (Fig. 2a). In this modified study population (n = 58), plasma DNA levels of >110 ng/mL were still associated with significantly increased D-dimer (Fig. 5e).
Effect of TF PCA on clinical outcome
In contrast, no difference was found for mOS or OS, when AML patients were stratified according to the TF PCA level of intact PBMCs using either 735 AU/106 cells (corresponding to the 95th percentile of TF PCA levels within the control group) or 293 AU/106 cells (corresponding to the median TF PCA level within the patient cohort) as the cut-off value (Fig. 6c, d). While the presence of DIC at presentation did not adversely affect OS (Fig. 6e), it was significantly associated with early mortality (Fig. 6f).
In this study, we investigated PBMC-associated TF PCA in 69 patients with newly diagnosed AML and found that TF PCA expression beyond a critical level was inevitably associated with the evolution of decompensated DIC. Importantly, DIC was not restricted to APL patients, but also occurred in seven other patients, three of whom had acute (myelo)monocytic leukemia. To our knowledge, this is one of the largest prospective studies so far specifically addressing the determinants of systemic coagulation activation in newly diagnosed AML.
The increase in PBMC-associated TF PCA following cell disruption is consistent with the concept of cryptic TF that can be de-encrypted upon cellular activation or induction of apoptosis/necrosis . Previous studies have clearly shown that cryptic TF is entirely cell surface-expressed on (myelo)monocytic cells and not liberated from intracellular storage pools upon cell lysis [25–27]. Instead, negatively charged phospholipids (i.e. phosphatidylserine) exposed on the outer membrane leaflet act synergistically with thiol-disulfide exchange reactions to activate surface-expressed TF [28–30]. In this regard, our findings provide circumstantial clinical evidence that membrane alterations associated with apoptosis/necrosis indeed contribute to cellular TF activation in vivo, because serum LDH levels, a surrogate marker for leukemic cell turnover, significantly correlated with plasma D-dimer. Systemic coagulation activation in AML is thus, at least to a substantial extent, determined by the following three factors: specific upregulation of cellular TF PCA following leukemic transformation of hematopoietic stem cells, elevated numbers of circulating blasts, and a significant degree of spontaneous apoptosis/necrosis. In our study, none of the patients developed overt DIC after the implementation of induction chemotherapy, which may de-encrypt cellular TF through the above mechanisms [26, 29]. Interestingly, in DIC patient no. 11 (Table 2), the systemic coagulopathy resolved during phases of AML remission, but recurred simultaneously with fulminant AML relapse, suggesting that the procoagulant phenotype of myeloblasts may be preserved despite intensive anti-leukemic therapy, including allogenic hematopoietic stem cell transplantation.
Our findings also point to a role of circulating TF-bearing MPs in the pathogenesis of AML-associated DIC, which has most recently been suggested by other experimental and clinical observations [31–33]. Shedding of MPs typically results from cellular activation or apoptosis, but may occur spontaneously in solid cancers and hematological malignancies . Although MP-associated TF PCA was more frequently detected in DIC as compared to non-DIC patients, our findings do not allow the conclusion that shedding of TF-bearing MPs alone was sufficient to cause overt DIC in newly diagnosed AML. However, caution is warranted when comparing results of different studies due to a lack of standardized assays to measure MP TF.
The finding that plasma TF antigen was significantly increased in DIC as compared to non-DIC patients and healthy controls may be interpreted in favor of our conclusion that TF is an important determinant of DIC evolution in newly diagnosed AML. It is important to note, however, that solid-phase immunoassays may preferentially capture soluble (i.e. truncated) TF, which is functionally inactive, rather than MP-associated TF. Furthermore, there is concern about a lack of specificity when using human plasma in commercial TF ELISAs, which may result in inappropriately high background signals [35, 36]. Nevertheless, in our study, plasma TF antigen was specifically upregulated in patients with DIC (Fig. 4c). Because the commercial TF ELISA used in our study does not detect alternatively spliced TF (unpublished data), future studies should therefore investigate, if proteolytic degradation of full-length TF by enzymes liberated from dying myeloblasts represents a novel mechanism of controlling the extrinsic coagulation pathway in newly diagnosed AML. Taken together, functional assays are more sensitive and specific than ELISAs in detecting minute amounts of biologically active TF, but TF immunoassays may provide useful complementary information in complex disease states.
An important finding of our study is that significant systemic coagulation activation, as indicated by excessively elevated plasma D-dimer, may occur in the absence of TF PCA overexpression by PBMCs. In fact, three of the eleven DIC patients (27%) had TF PCA levels below the threshold values of 2,500 AU/106 cells for intact and 8,000 AU/106 cells for disrupted PBMCs (Fig. 2). All of these patients had quite high numbers of circulating blasts, but two of them had only moderately increased serum LDH levels (Table 2). These observations point to alternative cellular and molecular pathways contributing to systemic coagulation in newly diagnosed AML. In this regard, negatively charged polymers such as polyphosphates or nucleic acids (i.e. RNA and DNA) have recently been identified as key mediators of intrinsic contact pathway activation in vivo . Consistent with a highly aggressive hematological malignancy leading to substantial spontaneous cell death, we found significantly increased levels of cell-free plasma DNA in the AML patient cohort. Furthermore, DNA levels correlated with plasma D-dimer and serum LDH. Even when the seven DIC patients with exceedingly high PBMC-associated TF PCA were excluded, levels of cell-free plasma DNA were associated with the degree of systemic coagulation activation (Fig. 5e). These findings may be regarded as circumstantial clinical evidence that liberation of DNA from apoptotic/necrotic AML blasts indeed contributes to intravascular thrombin generation through contact activation of factor XII  and may thus stimulate further research into the role of the intrinsic coagulation pathway in AML-associated coagulopathies. It has to be noted, however, that we did not specifically consider the contribution of cytoplasmic RNA , which may be liberated from dying cells at an earlier stage than nuclear DNA and which may be more closely correlated with serum LDH levels. Nevertheless, DNA-mediated activation of factor XII could explain why other studies did not find a significant contribution of the TF-dependent coagulation pathway to systemic coagulation activation in various hematological malignancies, including AML [9, 10]. Another potential mediator of PCA in AML is cancer procoagulant (CP), a cysteine proteinase that activates factor X independently of factor VIIa (FVIIa) , although more recent studies have questioned a predominant role of CP in paraneoplastic coagulation activation .
In solid malignancies, TF expression has been linked to tumor angiogenesis. In particular, TF has been shown to regulate VEGF production via its cytoplasmic domain , and TF-FVIIa-mediated cell signaling through cleavage of protease-activated receptor-2 (PAR-2) is crucial to neoplastic blood vessel formation . Although such a relationship has also been postulated for hematological malignancies [43–45], our findings do not support an obvious association between TF PCA expression and VEGF secretion by isolated PBMCs in newly diagnosed AML. It has to be noted, however, that TF PCA, as measured in our study, is not directly coupled to TF signaling functions, because cryptic (i.e. non-coagulant) TF still binds FVIIa and thus retains its ability to activate PAR-2 . Furthermore, measurement of ex vivo VEGF production by isolated PBMCs may not adequately reflect bone marrow microvessel density, which is also likely dependent on additional angiogenic growth factors (e.g. bFGF, HGF) not addressed in our study .
Patients presenting with DIC had a higher probability of early death (Fig. 6f). In this regard, our observation that TF PCA of both intact and disrupted PBMCs was associated with the presence of DIC may point to a prognostic role of TF in newly diagnosed AML. However, using either the upper limit of normal or the median TF PCA level of intact PBMCs as an arbitrary cut-off value, we did not observe an effect of increased TF PCA expression on median or OS in our patient cohort.
Our study has several limitations. First, although the total patient cohort is one of the largest so far, the generalizability of conclusions is still limited by the relatively small sample size of DIC patients. Likewise, much larger studies may be required to define the true impact of leukemic cell TF PCA expression on clinical outcome in newly diagnosed AML. Second, we used a qualitative TGA to measure MP-associated TF PCA. Although this assay may adequately mirror TF-driven coagulation activation in a plasma environment, quantitative assays such as a previously described chromogenic FXa generation assay  may provide more subtle information on the role of TF-bearing MPs in AML-associated DIC. Third, the impact of induction chemotherapy or treatment with all-trans retinoic acid on TF PCA expression and MP shedding was not addressed in our study. Finally, albeit novel, our findings on the association of cell-free DNA with plasma D-Dimer are rather descriptive, and mechanistic studies with functional readouts and different methods of DNA isolation and quantification are thus required to further define the role of intrinsic contact pathway activation in newly diagnosed AML.
Our study clearly shows that PBMC-associated TF PCA expression beyond a threshold level inevitably results in decompensated DIC in patients with newly diagnosed AML. While shedding of TF-bearing MPs is likely involved in the pathophysiology of AML-associated coagulopathy, additional (i.e. TF-independent) pathways contribute to systemic coagulation activation and DIC evolution. Of these pathways, liberation of cell-free DNA may be a novel mediator of intrinsic contact pathway activation in this hematological malignancy.
The study protocol was approved by the ethics committee of the city of Hamburg, Germany (no. OB-059/05), and the study was conducted in accordance with the second Declaration of Helsinki. All patients and controls provided written informed consent.
Patients were eligible if they had been admitted to the University Medical Center Hamburg-Eppendorf, Germany, for diagnostic work-up and subsequent treatment of presumed AML, which was confirmed by standard cytological, cytogenetic, and immunophenotypic criteria in 69 patients (Table 1). In five and seven patients, however, the final diagnoses were ALL or MDS, respectively. These patients served as additional reference groups for the analysis of PBMC-associated TF PCA (see below). The ALL patient cohort comprised four females and one male (mean age, 37 ± 14 years), and the MDS patient cohort comprised three females and four males (65 ± 9 years). The group of healthy controls (n = 10) included four females and six males (54 ± 18 years). Although consecutive patient enrollment was not feasible for logistic or consenting reasons, patients were enrolled on a random basis between August 2005 and November 2014, thus grossly representing the population of AML patients treated at our institution.
Patients had to be at least 18 years of age with no clinical and laboratory evidence for acute bacterial or viral infections or severe hepatic or renal dysfunction. Major surgical procedures within the preceding 4 weeks and any systemic anticoagulation prior to study enrollment were exclusion criteria.
Blood sampling and processing
All blood samples were taken before the initiation of specific anti-leukemic therapy. Venous blood was drawn by puncture of an antecubital vein or through a central venous catheter into plastic tubes prefilled with either 3.2% (0.109 M) sodium citrate or lithium heparin. Citrate-anticoagulated whole blood was centrifuged for 18 min at 4,000 rpm (1,200×g) to obtain platelet-poor plasma, which was snap-frozen in liquid nitrogen and stored in aliquots at −80°C until analysis. Heparin-anticoagulated whole blood was used to isolate peripheral blood mononuclear cells (PBMCs) as described below.
Measurement of plasma D-dimer and thrombin–antithrombin (TAT) complexes
Plasma D-dimer and TAT complexes were quantified using the Innovance™ D-dimer test on a BCS™ coagulation analyzer and the Enzygnost™ TAT micro kit, respectively (Siemens Healthcare).
Isolation of PBMCs
PBMCs were isolated from heparinized whole blood by density gradient centrifugation on Ficoll-Hypaque (Pharmacia) as previously described . Cells were washed in phosphate-buffered saline (PBS), adjusted to 1 × 106/mL, and immediately analyzed for TF procoagulant activity (PCA).
Measurement of cellular TF PCA
A previously described single-stage clotting assay was used to measure TF-specific PCA in PBMCs that were either left intact or disrupted by repeated freeze-thawing . Briefly, 100 µL of cell suspension (1 × 106/mL) were incubated with 100 µL of normal human plasma (NHP) (HemosIL™; Instrumentation Laboratory) in the cuvettes of a KC10 coagulation instrument (Amelung) for 2 min at 37°C. Following the addition of CaCl2 (final concentration, 5 mM), times until fibrin clot formation were recorded. All measurements were carried out in triplicates in the presence of 30 µg/mL inhibitory TF monoclonal antibody (#4509; American Diagnostica) or control IgG (Sigma). Clotting times were converted into arbitrary PCA units (AU) by reference to a standard curve obtained by serial dilutions of lipidated recombinant human TF (Innovin™; Dade Behring).
Measurement of microparticle-associated TF PCA
Plasma microparticles (MPs) were isolated by centrifugation at 100,000×g for 90 min at 10°C. Pellets were resuspended in the original volume with PBS. MP-associated TF activity was measured by a TGA according to the method developed by Hemker [48, 49]. Briefly, 20 µL of MP suspension were added, along with 20 µL of a mixture containing CaCl2 and the fluorogenic substrate Z-GGA-AMC-HCl (Bachem BioSciences), to 80 µL NHP in the presence of 25 µg/mL corn trypsin inhibitor (Enzyme Research Laboratories). Thrombin generation was measured over a period of 90 min using a Synergy 2 fluorometer (BioTek). MP suspensions were added as the only source of TF and phospholipids to initiate coagulation. Inhibitory TF antibody H36 (50 µg/mL) (Sunol Molecular) was employed to verify TF specificity.
Measurement of plasma TF antigen
Plasma TF antigen was measured using the Quantikine™ enzyme-linked immunosorbent assay (ELISA) (R&D Systems) according to the manufacturer’s instructions.
Measurement of VEGF antigen in plasma and culture supernatant
The Quantikine™ ELISA (R&D Systems) was used to measure vascular endothelial growth factor (VEGF) antigen levels in plasma samples and culture supernatants. Supernatants were prepared by incubating isolated PBMCs (1 × 106/mL) for 24 h at 37°C and 5% CO2 in RPMI culture medium in the presence of 10% fetal calf serum. Cells were removed by centrifugation and supernatants stored at −80°C until analysis.
Quantification of cell-free plasma DNA
Plasma DNA was quantified based on a previously described method . Briefly, 2 µL of plasma were diluted in 98 µL of PBS containing 0.1% bovine serum albumin. Diluted plasma was then mixed with 100 µL PBS containing Sytox™ Green nucleic acid stain (Invitrogen) at a final concentration of 2 µM to label DNA fluorescently. Fluorescence was recorded using MTP reader (Tecan) with a 485 nm excitation and 535 nm emission filter set. Autofluorescence was considered as background and determined in samples mixed with PBS without Sytox™ Green. DNA concentrations were calculated based on a standard curve obtained by known concentrations of DNA.
Normally and non-normally distributed data were presented as mean ± standard deviation and median with (interquartile) range, respectively. Differences between two groups were analyzed using the two-sided Student’s t test or the Mann–Whitney U test. Differences between multiple groups were analyzed using the Kruskal–Wallis test. Categorical data were analyzed using the Fisher’s exact test. Correlation coefficients were according the method of Spearman. Kaplan–Meier survival curves were compared using the log-rank (Mantel–Cox) test. All analyses were carried out using GraphPad Prism™ software. A P value of <0.05 was considered statistically significant.
acute coronary syndrome
acute lymphoblastic leukemia
acute myeloid leukemia
acute promyelocytic leukemia
basic fibroblast growth factor
disseminated intravascular coagulation
enzyme-linked immunosorbent assay
hepatocyte growth factor
International Society on Thrombosis and Haemostasis
median overall survival
neutrophil extracellular traps
normal human plasma
peripheral blood mononuclear cells
Scientific and Standardization Committee
thrombin generation assay
vascular endothelial growth factor
CD recruited patients, collected and interpreted clinical data, and critically revised the manuscript. AA designed experiments, interpreted data, and co-wrote the manuscript. BS and MJA performed experiments and analyzed data. TF designed experiments, analyzed data, and critically revised the manuscript. MD performed experiments, analyzed data, and critically revised the manuscript. JLF and CB oversaw the study, contributed to data interpretation, and critically revised the manuscript. FL designed the study, analyzed data, and wrote the first draft of the manuscript. All authors read and approved the final manuscript.
This work was supported by grants from the Hamburger Krebsgesellschaft e. V. and the Eppendorfer Krebs- und Leukämiehilfe e. V. to FL and the Deutsche Forschungsgemeinschaft (INST 152/624) and a Marie Curie Fellowship (ESR 628264) to TAF.
Compliance with ethical guidelines
Competing interests The authors declare that they have no competing interests.
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- Franchini M, Frattini F, Crestani S, Bonfanti C. Bleeding complications in patients with hematologic malignancies. Semin Thromb Hemost. 2013;39(1):94–100. doi:10.1055/s-0032-1331154.PubMedGoogle Scholar
- Colombo R, Gallipoli P, Castelli R. Thrombosis and hemostatic abnormalities in hematological malignancies. Clin Lymphoma Myeloma Leuk. 2014;14(6):441–50. doi:10.1016/j.clml.2014.05.003.PubMedView ArticleGoogle Scholar
- Kwaan HC. Double hazard of thrombophilia and bleeding in leukemia. Hematol Am Soc Hematol Educ Program. 2007;151–157. doi:10.1182/asheducation-2007.1.151.
- Kwaan HC, Cull EH. The coagulopathy in acute promyelocytic leukaemia—what have we learned in the past twenty years. Best Pract Res Clin Haematol. 2014;27(1):11–8. doi:10.1016/j.beha.2014.04.005.PubMedView ArticleGoogle Scholar
- Andoh K, Kubota T, Takada M, Tanaka H, Kobayashi N, Maekawa T. Tissue factor activity in leukemia cells. Special reference to disseminated intravascular coagulation. Cancer. 1987;59(4):748–54.PubMedView ArticleGoogle Scholar
- Bauer KA, Conway EM, Bach R, Konigsberg WH, Griffin JD, Demetri G. Tissue factor gene expression in acute myeloblastic leukemia. Thromb Res. 1989;56(3):425–30.PubMedView ArticleGoogle Scholar
- Tanaka M, Yamanishi H. The expression of tissue factor antigen and activity on the surface of leukemic cells. Leuk Res. 1993;17(2):103–11.PubMedView ArticleGoogle Scholar
- Lopez-Pedrera C, Jardi M, del Mar Malagon M, Ingles-Esteve J, Dorado G, Torres A, et al. Tissue factor (TF) and urokinase plasminogen activator receptor (uPAR) and bleeding complications in leukemic patients. Thromb Haemost. 1997;77(1):62–70.PubMedGoogle Scholar
- Negaard HF, Iversen PO, Ostenstad B, Iversen N, Holme PA, Sandset PM. Hypercoagulability in patients with haematological neoplasia: no apparent initiation by tissue factor. Thromb Haemost. 2008;99(6):1040–8. doi:10.1160/TH07-09-0541.PubMedGoogle Scholar
- Negaard HF, Iversen PO, Ostenstad B, Mowinckel MC, Sandset PM. Increased acquired activated protein C resistance in unselected patients with hematological malignancies. J Thromb Haemost. 2008;6(9):1482–7. doi:10.1111/j.1538-7836.2008.03060.x.PubMedView ArticleGoogle Scholar
- Taylor FB Jr, Toh CH, Hoots WK, Wada H, Levi M. Scientific Subcommittee on Disseminated Intravascular Coagulation of the International Society on Thrombosis and Haemostasis (ISTH). Towards definition, clinical and laboratory criteria, and a scoring system for disseminated intravascular coagulation. Thromb Haemost. 2001;86(5):1327–30.PubMedGoogle Scholar
- Langer F, Bokemeyer C. Crosstalk between cancer and haemostasis. Implications for cancer biology and cancer-associated thrombosis with focus on tissue factor. Hamostaseologie. 2012;32(2):95–104. doi:10.5482/ha-1160.PubMedView ArticleGoogle Scholar
- Fiedler W, Graeven U, Ergun S, Verago S, Kilic N, Stockschlader M, et al. Vascular endothelial growth factor, a possible paracrine growth factor in human acute myeloid leukemia. Blood. 1997;89(6):1870–5.PubMedGoogle Scholar
- Aguayo A, Estey E, Kantarjian H, Mansouri T, Gidel C, Keating M, et al. Cellular vascular endothelial growth factor is a predictor of outcome in patients with acute myeloid leukemia. Blood. 1999;94(11):3717–21.PubMedGoogle Scholar
- Hussong JW, Rodgers GM, Shami PJ. Evidence of increased angiogenesis in patients with acute myeloid leukemia. Blood. 2000;95(1):309–13.PubMedGoogle Scholar
- Aguayo A, Kantarjian H, Manshouri T, Gidel C, Estey E, Thomas D, et al. Angiogenesis in acute and chronic leukemias and myelodysplastic syndromes. Blood. 2000;96(6):2240–5.PubMedGoogle Scholar
- Fuchs TA, Brill A, Duerschmied D, Schatzberg D, Monestier M, Myers DD Jr, et al. Extracellular DNA traps promote thrombosis. Proc Natl Acad Sci USA. 2010;107(36):15880–5. doi:10.1073/pnas.1005743107.PubMed CentralPubMedView ArticleGoogle Scholar
- Massberg S, Grahl L, von Bruehl ML, Manukyan D, Pfeiler S, Goosmann C, et al. Reciprocal coupling of coagulation and innate immunity via neutrophil serine proteases. Nat Med. 2010;16(8):887–96. doi:10.1038/nm.2184.PubMedView ArticleGoogle Scholar
- Demers M, Krause DS, Schatzberg D, Martinod K, Voorhees JR, Fuchs TA, et al. Cancers predispose neutrophils to release extracellular DNA traps that contribute to cancer-associated thrombosis. Proc Natl Acad Sci USA. 2012;109(32):13076–81. doi:10.1073/pnas.1200419109.PubMed CentralPubMedView ArticleGoogle Scholar
- Diaz JA, Fuchs TA, Jackson TO, Kremer Hovinga JA, Lammle B, Henke PK, et al. Plasma DNA is elevated in patients with deep vein thrombosis. J Vasc Surg Venous Lymphat Disord. 2013;1(4). doi:10.1016/j.jvsv.2012.12.002.
- van Montfoort ML, Stephan F, Lauw MN, Hutten BA, Van Mierlo GJ, Solati S, et al. Circulating nucleosomes and neutrophil activation as risk factors for deep vein thrombosis. Arterioscler Thromb Vasc Biol. 2013;33(1):147–51. doi:10.1161/ATVBAHA.112.300498.PubMedView ArticleGoogle Scholar
- Fuchs TA, Kremer Hovinga JA, Schatzberg D, Wagner DD, Lammle B. Circulating DNA and myeloperoxidase indicate disease activity in patients with thrombotic microangiopathies. Blood. 2012;120(6):1157–64. doi:10.1182/blood-2012-02-412197.PubMed CentralPubMedView ArticleGoogle Scholar
- Kannemeier C, Shibamiya A, Nakazawa F, Trusheim H, Ruppert C, Markart P, et al. Extracellular RNA constitutes a natural procoagulant cofactor in blood coagulation. Proc Natl Acad Sci USA. 2007;104(15):6388–93. doi:10.1073/pnas.0608647104.PubMed CentralPubMedView ArticleGoogle Scholar
- Bach RR. Tissue factor encryption. Arterioscler Thromb Vasc Biol. 2006;26(3):456–61. doi:10.1161/01.ATV.0000202656.53964.04.PubMedView ArticleGoogle Scholar
- Drake TA, Ruf W, Morrissey JH, Edgington TS. Functional tissue factor is entirely cell surface expressed on lipopolysaccharide-stimulated human blood monocytes and a constitutively tissue factor-producing neoplastic cell line. J Cell Biol. 1989;109(1):389–95.PubMedView ArticleGoogle Scholar
- Langer F, Amirkhosravi A, Loges S, Meyer T, Eifrig B, Hossfeld DK, et al. An in vitro study on the mechanisms of coagulation activation in acute myelogenous leukemia (AML): role of tissue factor regulation by cytotoxic drugs and GM-CSF. Thromb Haemost. 2004;92(5):1136–46. doi:10.1267/THRO040511136.PubMedGoogle Scholar
- Langer F, Spath B, Fischer C, Stolz M, Ayuk FA, Kroger N, et al. Rapid activation of monocyte tissue factor by antithymocyte globulin is dependent on complement and protein disulfide isomerase. Blood. 2013;121(12):2324–35. doi:10.1182/blood-2012-10-460493.PubMed CentralPubMedView ArticleGoogle Scholar
- Bach RR, Moldow CF. Mechanism of tissue factor activation on HL-60 cells. Blood. 1997;89(9):3270–6.PubMedGoogle Scholar
- Boles JC, Williams JC, Hollingsworth RM, Wang JG, Glover SL, Owens AP III, et al. Anthracycline treatment of the human monocytic leukemia cell line THP-1 increases phosphatidylserine exposure and tissue factor activity. Thromb Res. 2012;129(2):197–203. doi:10.1016/j.thromres.2011.06.022.PubMedView ArticleGoogle Scholar
- Langer F, Ruf W. Synergies of phosphatidylserine and protein disulfide isomerase in tissue factor activation. Thromb Haemost. 2014;111(4):590–7. doi:10.1160/TH13-09-0802.PubMed CentralPubMedView ArticleGoogle Scholar
- Ma G, Liu F, Lv L, Gao Y, Su Y. Increased promyelocytic-derived microparticles: a novel potential factor for coagulopathy in acute promyelocytic leukemia. Ann Hematol. 2013;92(5):645–52. doi:10.1007/s00277-013-1676-6.PubMedView ArticleGoogle Scholar
- Gheldof D, Mullier F, Bailly N, Devalet B, Dogne JM, Chatelain B, et al. Microparticle bearing tissue factor: a link between promyelocytic cells and hypercoagulable state. Thromb Res. 2014;133(3):433–9. doi:10.1016/j.thromres.2013.11.008.PubMedView ArticleGoogle Scholar
- Thaler J, Pabinger I, Sperr WR, Ay C. Clinical evidence for a link between microparticle-associated tissue factor activity and overt disseminated intravascular coagulation in patients with acute myelocytic leukemia. Thromb Res. 2014;133(3):303–5. doi:10.1016/j.thromres.2013.12.029.PubMedView ArticleGoogle Scholar
- Owens AP III, Mackman N. Microparticles in hemostasis and thrombosis. Circ Res. 2011;108(10):1284–97. doi:10.1161/CIRCRESAHA.110.233056.PubMed CentralPubMedView ArticleGoogle Scholar
- Parhami-Seren B, Butenas S, Krudysz-Amblo J, Mann KG. Immunologic quantitation of tissue factors. J Thromb Haemost. 2006;4(8):1747–55.PubMedView ArticleGoogle Scholar
- Lee RD, Barcel DA, Williams JC, Wang JG, Boles JC, Manly DA, et al. Pre-analytical and analytical variables affecting the measurement of plasma-derived microparticle tissue factor activity. Thromb Res. 2012;129(1):80–5. doi:10.1016/j.thromres.2011.06.004.PubMed CentralPubMedView ArticleGoogle Scholar
- Mackman N. New insights into the mechanisms of venous thrombosis. J Clin Investig. 2012;122(7):2331–6. doi:10.1172/JCI60229.PubMed CentralPubMedView ArticleGoogle Scholar
- von Bruhl ML, Stark K, Steinhart A, Chandraratne S, Konrad I, Lorenz M, et al. Monocytes, neutrophils, and platelets cooperate to initiate and propagate venous thrombosis in mice in vivo. J Exp Med. 2012;209(4):819–35. doi:10.1084/jem.20112322.View ArticleGoogle Scholar
- Falanga A, Alessio MG, Donati MB, Barbui T. A new procoagulant in acute leukemia. Blood. 1988;71(4):870–5.PubMedGoogle Scholar
- Kazmierczak M, Lewandowski K, Wojtukiewicz MZ, Turowiecka Z, Kolacz E, Lojko A, et al. Cancer procoagulant in patients with adenocarcinomas. Blood Coagul Fibrinolysis. 2005;16(8):543–7.PubMedView ArticleGoogle Scholar
- Abe K, Shoji M, Chen J, Bierhaus A, Danave I, Micko C, et al. Regulation of vascular endothelial growth factor production and angiogenesis by the cytoplasmic tail of tissue factor. Proc Natl Acad Sci USA. 1999;96(15):8663–8.PubMed CentralPubMedView ArticleGoogle Scholar
- Ruf W, Disse J, Carneiro-Lobo TC, Yokota N, Schaffner F. Tissue factor and cell signalling in cancer progression and thrombosis. J Thromb Haemost. 2011;9(Suppl 1):306–15. doi:10.1111/j.1538-7836.2011.04318.x.PubMed CentralPubMedView ArticleGoogle Scholar
- Lopez-Pedrera C, Barbarroja N, Dorado G, Siendones E, Velasco F. Tissue factor as an effector of angiogenesis and tumor progression in hematological malignancies. Leukemia. 2006;20(8):1331–40. doi:10.1038/sj.leu.2404264.PubMedView ArticleGoogle Scholar
- Ribatti D. Tissue factor in hematological malignancies. Leukemia. 2006;20(8):1356–7. doi:10.1038/sj.leu.2404269.PubMedView ArticleGoogle Scholar
- Barbarroja N, Aristides-Torres L, Hernandez V, Martin C, Dorado G, Torres A, et al. Coordinated deregulation of cellular receptors, proangiogenic factors and intracellular pathways in acute myeloid leukaemia. Leuk Lymphoma. 2007;48(6):1187–99. doi:10.1080/10428190701340616.PubMedView ArticleGoogle Scholar
- Ahamed J, Versteeg HH, Kerver M, Chen VM, Mueller BM, Hogg PJ, et al. Disulfide isomerization switches tissue factor from coagulation to cell signaling. Proc Natl Acad Sci USA. 2006;103(38):13932–7. doi:10.1073/pnas.0606411103.PubMed CentralPubMedView ArticleGoogle Scholar
- Langer F, Spath B, Haubold K, Holstein K, Marx G, Wierecky J, et al. Tissue factor procoagulant activity of plasma microparticles in patients with cancer-associated disseminated intravascular coagulation. Ann Hematol. 2008;87(6):451–7. doi:10.1007/s00277-008-0446-3.PubMedView ArticleGoogle Scholar
- Hemker HC, Giesen P, Al Dieri R, Regnault V, de Smedt E, Wagenvoord R, et al. Calibrated automated thrombin generation measurement in clotting plasma. Pathophysiol Haemost Thromb. 2003;33(1):4–15.PubMedView ArticleGoogle Scholar
- Hemker HC, Beguin S. Thrombin generation in plasma: its assessment via the endogenous thrombin potential. Thromb Haemost. 1995;74(1):134–8.PubMedGoogle Scholar