Next Article in Journal
Alcohol Induced Depression: Clinical, Biological and Genetic Features
Next Article in Special Issue
Epithelial Ovarian Cancer and the Immune System: Biology, Interactions, Challenges and Potential Advances for Immunotherapy
Previous Article in Journal
Clinical Profiles in Renal Patients with COVID-19
Previous Article in Special Issue
Role of Non-Coding RNAs in the Development of Targeted Therapy and Immunotherapy Approaches for Chronic Lymphocytic Leukemia
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
JCM
Volume 9
Issue 8
10.3390/jcm9082666
jcm-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Brief Report

The Antitumor Effect of Heparin is not Mediated by Direct NK Cell Activation

by
Gustavo R. Rossi
1,2,*,
Jenifer P. Gonçalves
1,
Timothy McCulloch
2,
Rebecca B. Delconte
3,4,5,
Robert J. Hennessy
3,4,
Nicholas D. Huntington
3,4,6,
Edvaldo S. Trindade
1,* and
Fernando Souza-Fonseca-Guimaraes
2,*
1
Cellular Biology Department, Federal University of Paraná, Curitiba, Paraná CEP 81351-980, Brazil
2
The University of Queensland Diamantina Institute, University of Queensland, Woolloongabba, QLD 4102, Australia
3
Division of Molecular Immunology, The Walter and Eliza Hall Institute of Medical Research, Parkville, VIC 3052, Australia
4
Department of Medical Biology, Faculty of Medicine, Dentistry and Health Sciences, University of Melbourne, Parkville, VIC 3010, Australia
5
Immunology Program, Memorial Sloan Kettering Cancer Center, New York, NY 10065, USA
6
Department of Biochemistry and Molecular Biology, Biomedicine Discovery Institute, Monash University, Clayton, VIC 3800, Australia
*
Authors to whom correspondence should be addressed.
J. Clin. Med. 2020, 9(8), 2666; https://doi.org/10.3390/jcm9082666
Submission received: 19 July 2020 / Revised: 7 August 2020 / Accepted: 11 August 2020 / Published: 18 August 2020
(This article belongs to the Special Issue Immuno-Oncology: Identification of Therapeutic Targets, Development of Novel Drugs and Improvement of Treatment Approaches for Cancer)
Browse Figures
Versions Notes

Abstract

:
Natural killer (NK) cells are innate lymphocytes responsible for the elimination of infected or transformed cells. The activation or inhibition of NK cells is determined by the balance of target cell ligand recognition by stimulatory and inhibitory receptors on their surface. Previous reports have suggested that the glycosaminoglycan heparin is a ligand for the natural cytotoxicity receptors NKp30, NKp44 (human), and NKp46 (both human and mouse). However, the effects of heparin on NK cell homeostasis and function remain unclear. Here, we show that heparin does not enhance NK cell proliferation or killing through NK cell activation. Alternatively, in mice models, heparin promoted NK cell survival in vitro and controlled B16-F10 melanoma metastasis development in vivo. In human NK cells, heparin promisingly increased interferon (IFN)-γ production in synergy with IL-12, although the mechanism remains elusive. Our data showed that heparin is not able to increase NK cell cytotoxicity.

1. Introduction

Immune checkpoint inhibitors have revolutionized cancer therapy by reactivating tumor-resident cytotoxic lymphocytes. Checkpoint inhibitors primarily block inhibitory pathways in tumor-resident T cells; however, interest in other effector populations, such as natural killer (NK) cells, is growing. NK cells possess an innate ability to detect cellular transformation and are key to cancer immunosurveillance, particularly in settings of metastasis (e.g., melanoma) or hematological cancers [1]. Therapeutic strategies for metastatic melanoma have been changing over time to achieve optimal outcomes, and as such, chemotherapy has been increasingly replaced with more targeted immunotherapies [2]. Current immunotherapy regimens for treating melanoma are based on high doses of proinflammatory cytokines (IL-2 or Interferon-α) [3] or monoclonal antibodies to block antitumor immune checkpoints and stimulate cytotoxic T lymphocytes (anti-CTLA-4L and anti-PD-1L) [4,5,6]. NK cells are emerging as targets for cancer immunotherapy due to many advantages. For instance, they present reduced risk of autoimmune disease compared to cytotoxic T lymphocytes [1]. Additionally, as innate lymphocytes that are poised to kill transformed or infected cells [7], NK cells do not require prior clonal selection and expansion by specific antigens [1]. Instead, NK cells have many stimulatory (e.g., NKG2D, NKp30, NKp44, NKp46, CD16) and inhibitory (e.g., PD-1, TIM3, TIGIT, KIR/Ly49, NKG2A) surface receptors that directly define their activation and cytotoxic state [8,9]. At the same time, cancer cells create a complex tumor microenvironment to evade immunosurveillance by NK cells [10], such as using the TGF-β superfamily to impair NK cell antitumor responses by suppressing their metabolism, killing capacity, and inducing tissue residency characteristics [11,12,13]. The discovery of new immune stimulators could overcome this immune suppression of NK cells by tumors.
Advanced-stage metastatic melanoma patients are at high risk of developing the clinical condition of cancer-associated thrombosis (CAT) [14], a major adverse effect that can often result in death of the patient [15]. The process starts with tumor cells ability to activate the coagulation cascade, leading to activation/production of Xa and VIIa factors, thrombin, and fibrin, resulting in platelet recruitment and culminating in thrombus formation [15,16]. The classic anticoagulant drug heparin [17] is used in oncology clinics to avoid thrombus in the bloodstream [18], where heparin-treated patients show increased survival, usually associated with a lower incidence of CAT [19]. However, the possible direct antitumor effects of heparin are multifactorial. Heparin may act by reducing the activity of extracellular matrix remodeling enzymes, such as heparanases and metalloproteases [20]. Aside from the inhibition of many coagulation cascade components, heparin binds to P-selectin on the surface of platelets, blocking their adhesion to tumor cells and making them more visible to the immune system [21]. The combination of such factors leads to reduction of metastasis in a number of animal models, such as colon and mammary cancer, melanoma, and adenocarcinoma [22,23,24,25]. Some reports suggest a potential interaction between heparin and NK cell stimulatory receptors, such as NKp30, NKp44 (human) and NKp46 (both human and mouse) [26,27,28]. However, whether these interactions can indeed lead to activation of NK cell antitumor responses is still unanswered. Herein, we investigated the hypothesis that heparin could activate NK cell antitumor responses by increasing their cytotoxic capacity against tumor cells.

2. Experimental Section

2.1. Ethics

Animal experiments followed the National Health and Medical Research Council (NHMRC) Code of Practice for the Care and Use of Animals for Scientific Purposes guidelines and were approved by the Animal Ethics Committees at both the Walter and Eliza Hall Institute (WEHI) and the University of Queensland Diamantina Institute (UQDI). All procedures performed in studies involving human participants were in accordance with the ethical standards of the Human Research Ethics Committee at WEHI and UQDI.

2.2. Heparin

Unfractionated heparin was purchased from BioIberia (Bacelona, Spain). For in vivo assays, heparin was dissolved in PBS (Gibco—Thermo Fisher Scientific, Waltham, MA, USA) (2.5 mg/mL), and for in vitro assays, heparin was dissolved in RPMI medium (Gibco) (5 mg/mL). Both solutions were sterilized by filtration using 0.22-µm syringe filters.

2.3. Mice

C57BL/6 (WT), Rag2−/−γc−/− (immunocompromised), or Ncr1−/− (NKp46-deficient) mice were bred and maintained under specific pathogen-free conditions at WEHI or UQDI. All animal experiments were performed using an age range of 8–12 weeks.

2.4. Cell Lines

B16-F10 murine melanoma and A375 human melanoma cells were maintained at 37 °C and 5% CO2 in DMEM (Gibco) supplemented with 10% fetal bovine serum (FBS) (Gibco), 1% GlutaMAX (Gibco), 1% non-essential amino acids (NEAA) (Gibco), 10 mM HEPES (Gibco), and 1% penicillin/streptomycin (Gibco). YAC-1 murine leukemia cells were cultured in RPMI-1640 supplemented with 10% FBS, 1% GlutaMAX, 10 mM HEPES, 1% NEAA, and 1% penicillin/streptomycin.

2.5. NK Cell Isolation and Culture

NK cells from spleens of WT and Ncr1−/− mice were isolated by organ maceration, followed by selection using a mouse NK cell isolation kit (Miltenyi Biotec, Bergisch Gladbach, Germany). For human NK cell isolation, peripheral blood mononuclear cells (PBMCs) were first isolated from fresh umbilical cord blood by Ficoll-Paque density (1.077 g/mL) centrifugation (Sigma-Aldrich, St. Louis, MO, USA). NK cells were enriched from resulting PBMCs by following negative selection using the EasySep Human NK Cell Isolation Kit (Stem Cell Technologies, Vancouver, BC, Canada). Mouse and human NK cells were maintained in RPMI 1640 media supplemented with 10% FBS, 1% sodium pyruvate, 1% Glutamax, 1% NEAA, 10 mM HEPES, 0.1% 2-mercaptoethanol (Gibco), 1% penicillin/streptomycin, and human rIL-15 (Peprotech, Cranbury, NJ, USA).

2.6. Tumor Model

B16-F10 cells (2 × 105) were injected intravenously via the lateral tail vein into C57BL/6 mice or (1 × 105) into Rag2−/−γc−/− recipients reconstituted with NK cells as previously described [29]. Briefly, fresh isolated NK cells from WT or Ncr1−/− (4 × 105) were injected via the lateral tail vein into Rag2−/−γc−/− mice, 12 h after tumor cell inoculation.
After 24 h of tumor cells injection, animals were treated with 10 mg/kg of heparin, with subcutaneous (sc) injections of 100 μL heparin solution (2.5 mg/mL) or PBS (control) every second day for 14 days. At the endpoint, lungs were harvested, washed twice in PBS, and fixed in Fekete’s solution overnight [30] to macroscopically count surface metastases.

2.7. NK Cell Proliferation Assay

Fresh isolated mouse NK cells were incubated with Cell Trace Violet (CTV) (Thermo Fisher Scientific) according to the manufacturer’s instructions, and 1 × 104 labeled cells were seeded into 96-well V-bottom plates (Corning Inc., Corning, NY, USA) in culture media (200 µL/well) supplemented with rIL-15 (50 ng/mL), with or without heparin (100 µg/mL). Time endpoints (0, 24, 48, 72, 96, and 120 h) were assessed on a BD FACS Verse cytometer (BD Biosciences, San Jose, CA, USA). Flow cytometry analysis was performed using FlowJo X (BD Bioscience) software, and division numbers were determined using the precursor cohort-based method [12,31].

2.8. IFN-γ Production

Human NK cells (1 × 104) were seeded into 96-well V-bottom plates in culture media (200 µL/well), containing rIL-15 (50 ng/mL) and rIL-18 (Miltenyi Biotec) (50 ng/mL), with or without heparin (1 or 100 µg/mL), and incubated for 24 h. IFN-γ quantification was performed on the culture supernatant using the ELISA human IFN-γ Kit (R&D Systems, Minneapolis, MN, USA), and compared to an analytical standard curve. As a positive control for IFN-γ production, a group was incubated with rIL-12 (Miltenyi Biotec) (10 pg/mL). Absorbance was measured using a VICTOR3 plate reader (PerkinElmer, Waltham, MA, USA).

2.9. Mouse Target: Effector Cell Co-Cultures

Target tumor cells (B16-F10 or YAC-1) were labeled with 15 µg/mL Calcein AM (Thermo Fisher Scientific) for 30 min at 37 °C, as previously described [32]. Murine NK cells were cultured for 24 h in media containing rIL-15 (20 ng/mL), with or without heparin (10 or 100 µg/mL), and then used to perform a 4 h co-culture assay with B16-F10 or YAC-1 labeled cells in different ratios in a 96-well round bottom microplate. The plate was then centrifuged (300× g for 5 min) and the supernatant was collected and transferred to opaque 96-well plates (PerkinElmer). Fluorescence emission was measured with a CLARIOstar microplate reader (BMG Labtech, Ortenberg, Germany).

2.10. Human Target: Effector Cell Co-Cultures

A375 melanoma cells were detached with TrypLE (Gibco) and co-cultured for 4 h with human NK cells previously stained with CTV and cultured for 24 h in media containing rIL-15 (50 ng/mL), with or without heparin (1 or 100 µg/mL), in a 4:1 ratio into a 96-well V-bottom microplate. Cells were stained with Fluorescein isothiocyanate (FITC)-conjugated Annexin V and propidium iodide (PI) (BD Biosciences) according to manufacturer’s instructions, and dying or dead cells were assessed on a BD FACS Verse cytometer. Flow cytometry analysis was performed using FlowJo software.

2.11. Statistical Analysis

Statistical analyses (as indicated in the Figure legends) were performed using GraphPad Prism 8 software (GraphPad Software, San Diego, CA, USA).

3. Results

3.1. Heparin Does Not Depend on NK Cells Activation to Reduce B16-F10 Lung Metastasis

To assess whether a heparin administration and treatment schedule could affect B16-F10 lung metastasis formation as previously suggested [33], C57BL/6 mice were intravenously injected with B16-F10 cells and treated with heparin (10 mg/kg) every second day for 14 days. Heparin-treated mice showed a 25% reduction in the number of visible metastases (Figure 1A). In vivo control of B16-F10-induced lung metastasis is largely NK cell dependent [34,35]. Therefore, we hypothesized that the metastases reduction in heparin-treated mice was due to NK cells activation since in silico analysis has predicted NKp46 as a potential receptor for heparin on NK cells [26,28]. To investigate that, we injected Rag2−/−γc−/− mice with B16-F10 cells, and reconstituted the mice with WT or NKp46-deficient (Figure 1B) NK cells after 12 h, followed by the same heparin treatment schedule as above. However, we failed to observe any differences on lung metastases regarding heparin treatment at the endpoint, suggesting that the interaction of NKp46 with heparin was not the responsible factor for reducing metastasis in this model.

3.2. Heparin Does Not Increase In Vitro Proliferation of Murine NK Cells

Murine splenic NK cells were exposed to heparin and assayed for cell proliferation kinetics as previously described [12,31]. Interestingly, while heparin does not appear to affect NK cell division rates (Figure 2A), using total cohort number analysis to estimate survival of NK cells [31], we observed that heparin was able to enhance the survival of NK cells in vitro (Figure 2B). Addition of heparin in cell cultures for enhanced manufacturing of NK cell products has previously been considered [36] as it is an effective replacement for stroma [37], and this might be because of the survival stimulus that we showed here.

3.3. Heparin Does not Increase the Killing Capacity of Murine or Human NK Cells

To further investigate whether heparin could affect NK cell effector functions such as cytotoxicity, murine NK cells were pre-treated with heparin for 24 h, and then co-cultured with B16-F10 or YAC-1 cells. No difference in NK cell killing capacity was observed when treated with heparin across different NK:target cell ratios (Figure 3A,B), suggesting that heparin has no potential for stimulating NK cell cytotoxicity in this system. Human NK cells were also cultured in the presence of heparin, then co-cultured with A375 human melanoma cells, and again, no difference in NK cell killing capacity was observed (Figure 3C).

3.4. Heparin Increases IL-12-Mediated IFN-γ Production in Human NK Cells

We next evaluated the potential activation of NK cell effector functions by heparin. Human NK cells were cultured in the presence of heparin for 24 h and the production of IFN-γ was evaluated. Heparin did not increase the production of IFN-γ by NK cells cultured with rIL-15 and rIL-18. However, in the presence of the stimulatory cytokine IL-12, which drives production of IFN-γ and activation of NK cells [1], heparin significantly further enhanced IFN-γ production by NK cells (Figure 4)

4. Discussion

Considering that the average cost for developing a new drug is now more than 1 billion US dollars [38], repurposing of “old” drugs to treat other diseases is an attractive proposal [39]. Heparin has been used in clinics since 1935, mainly due to its anticoagulant activity [17]. Considering that heparin may be a ligand for stimulatory receptors on NK cells (NKp30, NKp44 and NKp46), and it is currently used for NK cell product manufacturing purposes [36], in addition to other polysaccharides with potential to stimulate NK cells [40,41,42], we evaluated the capacity of heparin to stimulate and increase killing capacity of NK cells.
Our results showed that heparin can reduce lung colonization by B16-F10 cells, which is in accordance with the literature for different types of cancer [33]. However, we failed to observe a direct association of heparin, NK cells, and the activating receptor NKp46, reinforcing previous suggestions that the antimetastatic effect is actually mediated by a direct effect of heparin over the B16-F10 cells (as previously suggested by others [43,44,45]), rather than a promotion of NK cell cytotoxicity. Corroborating our data, we also did not observe increased killing capacity of NK cells against both murine and human tumor cells in our experimental in vitro conditions. Therefore, heparin antimetastatic activity is likely mainly related to inhibition of coagulation, heparanase, and P-selectin interactions [46], avoiding cancer cell activation of the coagulation cascade to recruit a protective layer of platelets, and increase inflammation and angiogenesis [14].
A classical outcome of NK cell activation is the production of IFN-γ [47]. Our results showed that heparin alone could not stimulate IFN-γ production. However, when human NK cells were simultaneously cultured with the pro-inflammatory cytokine IL-12 and heparin, enhanced IFN-γ production was observed. IL-12 has a heparin binding site on the p40 subunit [48,49], and thus this interaction could potentially enhance IL-12 effect on NK cells, providing an explanation for our observed results. Similarly, another study using the human NK cell line NK-92MI also showed an increase of IFN-γ in the presence of heparin and IL-12 [50]. This increased IFN-γ production by NK cells could be related to the interaction of IL-12 with heparin rather than a direct effect of heparin on NK cells through receptors such as NKp46.
Our results suggest that heparin is unlikely to be a direct stimulator of human or murine NK cell killing capacity. However, it is worth noting that the heparin binding sites in the stimulatory receptors (NKp30, NKp44, and NKp46) might have been already occupied by an endogenous ligand, such as heparan sulfate (which has a composition/structure very similar to heparin [51]) chains derived from the proteoglycan syndecan-4 [52]. If this is the case, then the externally added heparin cannot target its binding sites in order to activate the NK cells.
Despite its lack of direct action on stimulatory NK cell receptors, the mechanism behind the heparin antimetastatic effect still needs to be further explored. Whether heparin interacts with other cell types that could exert beneficial off-target effects on NK cells is an exciting avenue to explore and has the potential to enhance combination therapies with direct NK cell-stimulating antibodies or cytokines.

Author Contributions

G.R.R. conducted the experiments, analyzed and interpreted the data. T.M., R.B.D., R.J.H., and F.S.-F.-G. assisted with the performance of experiments. E.S.T., T.M., J.P.G., N.D.H., R.B.D., R.J.H., and F.S.-F.-G. assisted with data interpretation. G.R.R., J.P.G., and F.S.-F.-G. co-wrote the manuscript F.S.-F.-G., N.D.H., and E.S.T. supervised the study. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by project grants from the National Health and Medical Research Council (NHMRC) of Australia (#1140406 to F.S.-F.-G.) and Coordenação de Aperfeiçoamento de Pessoal de Nível Superior (CAPES) of Brazil (CAPES/PROCAD 2965/2014, Finance Code 001 to E.S.T.). F.S.-F.-G. was also supported by a grant #1158085 awarded through the Priority-driven Collaborative Cancer Research Scheme and funded by Cure Cancer Australia with the assistance of Cancer Australia. N.D.H. is a NHMRC CDF2 Fellow (1124788), a recipient of a Melanoma Research Grant from the Harry J. Lloyd Charitable Trust, Melanoma Research Alliance Young Investigator Award, Ian Potter Foundation equipment grant, and a CLIP grant from Cancer Research Institute. R.B.D. was supported by a Cancer Council Victoria postdoctoral fellowship and is currently a NHMRC Early Career Fellow (GNT1158615). G.R.R. and J.P.G. were supported by a CAPES Ph.D. scholarship (PDSE—88881.188501/2018-01 and 88882.382557/2019-01), and G.R.R. was also supported by a Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) scholarship (140637/2017-6).

Acknowledgments

We thank all the members of the Huntington, Guimaraes, and Trindade Laboratories for discussion, comments, and advice on this project; Tania Camilleri for mouse breeding, maintenance, genotyping, and technical support.

Conflicts of Interest

N.D.H. is a cofounder and shareholder in oNKo-Innate. F.S.-F.-G. is a consultant for Biotheus Inc. The other authors have declared no conflict of interest.

References

  1. Souza-Fonseca-Guimaraes, F.; Cursons, J.; Huntington, N.D. The Emergence of Natural Killer Cells as a Major Target in Cancer Immunotherapy. Trends Immunol. 2019, 40, 142–158. [Google Scholar] [CrossRef]
  2. Kozar, I.; Margue, C.; Rothengatter, S.; Haan, C.; Kreis, S. Many ways to resistance: How melanoma cells evade targeted therapies. Biochim. Biophys. Acta Rev. Cancer 2019, 1871, 313–322. [Google Scholar] [CrossRef]
  3. Maverakis, E.; Cornelius, L.; Bowen, G.; Phan, T.; Patel, F.; Fitzmaurice, S.; He, Y.; Burrall, B.; Duong, C.; Kloxin, A.; et al. Metastatic Melanoma—A Review of Current and Future Treatment Options. Acta Derm. Venereol. 2015, 95, 516–524. [Google Scholar] [CrossRef] [Green Version]
  4. Davey, R.J.; Westhuizen, A.; van der Bowden, N.A. Metastatic melanoma treatment: Combining old and new therapies. Crit. Rev. Oncol. Hematol. 2016, 98, 242–253. [Google Scholar] [CrossRef]
  5. Eggermont, A.M.M.; Robert, C. New drugs in melanoma: It’s a whole new world. Eur. J. Cancer 2011, 47, 2150–2157. [Google Scholar] [CrossRef]
  6. Zaidi, M.R.; Day, C.-P.; Merlino, G. From UVs to Metastases: Modeling Melanoma Initiation and Progression in the Mouse. J. Investig. Dermatol. 2008, 128, 2381–2391. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Vivier, E.; Raulet, D.H.; Moretta, A.; Caligiuri, M.A.; Zitvogel, L.; Lanier, L.L.; Yokoyama, W.M.; Ugolini, S. Innate or adaptive immunity? The example of natural killer cells. Science (80-) 2011, 331, 44–49. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Chiossone, L.; Dumas, P.-Y.; Vienne, M.; Vivier, E. Natural killer cells and other innate lymphoid cells in cancer. Nat. Rev. Immunol. 2018, 18, 671–688. [Google Scholar] [CrossRef] [PubMed]
  9. Huntington, N.D.; Cursons, J.; Rautela, J. The cancer–natural killer cell immunity cycle. Nat. Rev. Cancer 2020, 20, 437–454. [Google Scholar] [CrossRef]
  10. Rossi, G.; Trindade, E.; Souza-Fonseca-Guimaraes, F. Tumor microenvironment-associated extracellular matrix components regulate NK cell function. Front. Immunol. 2020, 11, 1–10. [Google Scholar] [CrossRef]
  11. Gao, Y.; Souza-Fonseca-Guimaraes, F.; Bald, T.; Ng, S.S.; Young, A.; Ngiow, S.F.; Rautela, J.; Straube, J.; Waddell, N.; Blake, S.J.; et al. Tumor immunoevasion by the conversion of effector NK cells into type 1 innate lymphoid cells. Nat. Immunol. 2017, 18, 1004–1015. [Google Scholar] [CrossRef] [PubMed]
  12. Rautela, J.; Dagley, L.F.; de Oliveira, C.C.; Schuster, I.S.; Hediyeh-Zadeh, S.; Delconte, R.B.; Cursons, J.; Hennessy, R.; Hutchinson, D.S.; Harrison, C.; et al. Therapeutic blockade of activin-A improves NK cell function and antitumor immunity. Sci. Signal. 2019, 12, eaat7527. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Viel, S.; Marçais, A.; Guimaraes, F.S.F.; Loftus, R.; Rabilloud, J.; Grau, M.; Degouve, S.; Djebali, S.; Sanlaville, A.; Charrier, E.; et al. TGF-β inhibits the activation and functions of NK cells by repressing the mTOR pathway. Sci. Signal. 2016, 9. [Google Scholar] [CrossRef] [PubMed]
  14. Sparsa, A.; Durox, H.; Doffoel-Hantz, V.; Munyangango, E.M.; Bédane, C.; Cendras, J.; Gantois, C.; Boulinguez, S.; Bonnetblanc, J.M. High prevalence and risk factors of thromboembolism in stage IV melanoma. J. Eur. Acad. Dermatol. Venereol. 2011, 25, 340–344. [Google Scholar] [CrossRef] [PubMed]
  15. Abdol, N.R.; Jones, G.; Bhandari, M.; Berndt, M.; Metharom, P. Cancer-Associated Thrombosis: An Overview of Mechanisms, Risk Factors, and Treatment. Cancers (Basel) 2018, 10, 380. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Falanga, A.; Panova-Noeva, M.; Russo, L. Procoagulant mechanisms in tumour cells. Best Pract. Res. Clin. Haematol. 2009, 22, 49–60. [Google Scholar] [CrossRef]
  17. Oduah, E.; Linhardt, R.; Sharfstein, S. Heparin: Past, Present, and Future. Pharmaceuticals 2016, 9, 38. [Google Scholar] [CrossRef]
  18. Borsig, L. Heparin as an Inhibitor of Cancer Progression. In Progress in Molecular Biology and Translational Science; Academic Press: Cambridge, MA, USA, 2010; Volume 1173, pp. 335–349. [Google Scholar]
  19. Tieken, C.; Versteeg, H.H. Anticoagulants versus cancer. Thromb. Res. 2016, 140, S148–S153. [Google Scholar] [CrossRef]
  20. Engelberg, H. Actions of heparin that may affect the malignant process. Cancer 1999, 85, 257–272. [Google Scholar] [CrossRef]
  21. Borsig, L.; Wong, R.; Feramisco, J.; Nadeau, D.R.; Varki, N.M.; Varki, A. Heparin and cancer revisited: Mechanistic connections involving platelets, P-selectin, carcinoma mucins, and tumor metastasis. Proc. Natl. Acad. Sci. USA 2001, 98, 3352–3357. [Google Scholar] [CrossRef] [Green Version]
  22. Stevenson, J.L.; Varki, A.; Borsig, L. Heparin attenuates metastasis mainly due to inhibition of P- and L-selectin, but non-anticoagulant heparins can have additional effects. Thromb. Res. 2007, 120, 107–111. [Google Scholar] [CrossRef]
  23. Lee, A.E.; Rogers, L.A.; Longcroft, J.M.; Jeffery, R.E. Reduction of metastasis in a murine mammary tumour model by heparin and polyinosinic-polycytidylic acid. Clin. Exp. Metastasis 1990, 8, 165–171. [Google Scholar] [CrossRef] [PubMed]
  24. Stevenson, J.L.; Choi, S.H.; Varki, A. Differential metastasis inhibition by clinically relevant levels of heparins—Correlation with selectin inhibition, not antithrombotic activity. Clin. Cancer Res. 2005, 11, 7003–7011. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Ludwig, R.J.; Boehme, B.; Podda, M.; Henschler, R.; Jager, E.; Tandi, C.; Boehncke, W.H.; Zollner, T.M.; Kaufmann, R.; Gille, J. Endothelial P-Selectin as a Target of Heparin Action in Experimental Melanoma Lung Metastasis. Cancer Res. 2004, 64, 2743–2750. [Google Scholar] [CrossRef] [Green Version]
  26. Hecht, M.L.; Rosental, B.; Horlacher, T.; Hershkovitz, O.; De Paz, J.L.; Noti, C.; Schauer, S.; Porgador, A.; Seeberger, P.H. Natural cytotoxicity receptors NKp30, NKp44 and NKp46 bind to different heparan sulfate/heparin sequences. J. Proteome Res. 2009, 8, 712–720. [Google Scholar] [CrossRef]
  27. Hershkovitz, O.; Jivov, S.; Bloushtain, N.; Zilka, A.; Landau, G.; Bar-Ilan, A.; Lichtenstein, R.G.; Campbell, K.S.; Van Kuppevelt, T.H.; Porgador, A. Characterization of the recognition of tumor cells by the natural cytotoxicity receptor, NKp44. Biochemistry 2007, 46, 7426–7436. [Google Scholar] [CrossRef]
  28. Zilka, A.; Landau, G.; Hershkovitz, O.; Bloushtain, N.; Bar-Ilan, A.; Benchetrit, F.; Fima, E.; Van Kuppevelt, T.H.; Gallagher, J.T.; Elgavish, S.; et al. Characterization of the heparin/heparan sulfate binding site of the natural cytotoxicity receptor NKp46. Biochemistry 2005, 44, 14477–14485. [Google Scholar] [CrossRef]
  29. Souza-Fonseca-Guimaraes, F.; Young, A.; Mittal, D.; Martinet, L.; Bruedigam, C.; Takeda, K.; Andoniou, C.E.; Degli-Esposti, M.A.; Hill, G.R.; Smyth, M.J. NK cells require IL-28R for optimal in vivo activity. Proc. Natl. Acad. Sci. USA 2015, 112, E2376–E2384. [Google Scholar] [CrossRef] [Green Version]
  30. Overwijk, W.W.; Restifo, N.P. B16 as a Mouse Model for Human Melanoma. Curr. Protoc. Immunol. 2001, 39, 20-1. [Google Scholar] [CrossRef]
  31. Hennessy, R.J.; Pham, K.; Delconte, R.; Rautela, J.; Hodgkin, P.D.; Huntington, N.D. Quantifying NK cell growth and survival changes in response to cytokines and regulatory checkpoint blockade helps identify optimal culture and expansion conditions. J. Leukoc. Biol. 2019, 105, 1341–1354. [Google Scholar] [CrossRef]
  32. Neri, S.; Mariani, E.; Meneghetti, A.; Cattini, L.; Facchini, A. Calcein-Acetyoxymethyl Cytotoxicity Assay: Standardization of a Method Allowing Additional Analyses on Recovered Effector Cells and Supernatants. Clin. Vaccine Immunol. 2001, 8, 1131–1135. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Borsig, L. Antimetastatic activities of heparins and modified heparins. Experimental evidence. Thromb. Res. 2010, 125, S66–S71. [Google Scholar] [CrossRef] [Green Version]
  34. Sathe, P.; Delconte, R.B.; Souza-Fonseca-Guimaraes, F.; Seillet, C.; Chopin, M.; Vandenberg, C.J.; Rankin, L.C.; Mielke, L.A.; Vikstrom, I.; Kolesnik, T.B.; et al. Innate immunodeficiency following genetic ablation of Mcl1 in natural killer cells. Nat. Commun. 2014, 5. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Krasnova, Y.; Putz, E.M.; Smyth, M.J.; Souza-Fonseca-Guimaraes, F. Bench to bedside: NK cells and control of metastasis. Clin. Immunol. 2017, 177, 50–59. [Google Scholar] [CrossRef]
  36. Chabannon, C.; Mfarrej, B.; Guia, S.; Ugolini, S.; Devillier, R.; Blaise, D.; Vivier, E.; Calmels, B. Manufacturing natural killer cells as medicinal products. Front. Immunol. 2016, 7, 1–9. [Google Scholar] [CrossRef]
  37. Dezell, S.A.; Ahn, Y.-O.; Spanholtz, J.; Wang, H.; Weeres, M.; Jackson, S.; Cooley, S.; Dolstra, H.; Miller, J.S.; Verneris, M.R. Natural Killer Cell Differentiation from Hematopoietic Stem Cells: A Comparative Analysis of Heparin- and Stromal Cell–Supported Methods. Biol. Blood Marrow Transplant. 2012, 18, 536–545. [Google Scholar] [CrossRef] [Green Version]
  38. DiMasi, J.A.; Grabowski, H.G.; Hansen, R.W. Innovation in the pharmaceutical industry: New estimates of R&D costs. J. Health Econ. 2016, 47, 20–33. [Google Scholar]
  39. Pushpakom, S.; Iorio, F.; Eyers, P.A.; Escott, K.J.; Hopper, S.; Wells, A.; Doig, A.; Guilliams, T.; Latimer, J.; McNamee, C.; et al. Drug repurposing: Progress, challenges and recommendations. Nat. Rev. Drug Discov. 2019, 18, 41–58. [Google Scholar] [CrossRef]
  40. Lee, D.-Y.; Park, C.W.; Lee, S.J.; Park, H.-R.; Kim, S.H.; Son, S.-U.; Park, J.; Shin, K.-S. Anti-Cancer Effects of Panax ginseng Berry Polysaccharides via Activation of Immune-Related Cells. Front. Pharmacol. 2019, 10, 1–11. [Google Scholar] [CrossRef] [Green Version]
  41. Shin, M.-S.; Hwang, S.-H.; Yoon, T.-J.; Kim, S.H.; Shin, K.-S. Polysaccharides from ginseng leaves inhibit tumor metastasis via macrophage and NK cell activation. Int. J. Biol. Macromol. 2017, 103, 1327–1333. [Google Scholar] [CrossRef]
  42. Park, H.R.; Hwang, D.; Hong, H.D.; Shin, K.S. Antitumor and antimetastatic activities of pectic polysaccharides isolated from persimmon leaves mediated by enhanced natural killer cell activity. J. Funct. Foods 2017, 37, 460–466. [Google Scholar] [CrossRef]
  43. Koçak, F.E.; Erdoğan, E.; Ozyıgıt, F.; Yerlıkaya, A. Evaluation of antiproliferative and antimetastatic effects of heparin and erythropoietin on B16f10 melanoma cell line. Cell. Mol. Biol. (Noisy-le-grand) 2013, 59, OL1894–OL1898. [Google Scholar]
  44. Zhang, C.; Liu, Y.; Gao, Y.; Shen, J.; Zheng, S.; Wei, M.; Zeng, X. Modified heparins inhibit integrin α IIb β 3 mediated adhesion of melanoma cells to platelets in vitro and in vivo. Int. J. Cancer 2009, 125, 2058–2065. [Google Scholar] [CrossRef] [PubMed]
  45. Fritzsche, J.; Simonis, D.; Bendas, G. Melanoma cell adhesion can be blocked by heparin in vitro: Suggestion of VLA-4 as a novel target for antimetastatic approaches. Thromb. Haemost. 2008, 100, 1166–1175. [Google Scholar]
  46. Niers, T.M.H.; Klerk, C.P.W.; DiNisio, M.; Van Noorden, C.J.F.; Büller, H.R.; Reitsma, P.H.; Richel, D.J. Mechanisms of heparin induced anti-cancer activity in experimental cancer models. Crit. Rev. Oncol. Hematol. 2007, 61, 195–207. [Google Scholar] [CrossRef]
  47. Souza-Fonseca-Guimaraes, F.; Adib-Conquy, M.; Cavaillon, J.M. Natural killer (NK) cells in antibacterial innate immunity: Angels or devils? Mol. Med. 2012, 18, 270–285. [Google Scholar] [CrossRef]
  48. Garnier, P.; Mummery, R.; Forster, M.J.; Mulloy, B.; Gibbs, R.V.; Rider, C.C. The localisation of the heparin binding sites of human and murine interleukin-12 within the carboxyterminal domain of the P40 subunit. Cytokine 2018, 110, 159–168. [Google Scholar] [CrossRef]
  49. Hasan, M.; Najjam, S.; Gordon, M.Y.; Gibbs, R.V.; Rider, C.C. IL-12 is a heparin-binding cytokine. J. Immunol. 1999, 162, 1064–1070. [Google Scholar]
  50. Jayanthi, S.; Koppolu, B.P.; Nguyen, K.G.; Smith, S.G.; Felber, B.K.; Kumar, T.K.S.; Zaharoff, D.A. Modulation of Interleukin-12 activity in the presence of heparin. Sci. Rep. 2017, 7, 5360. [Google Scholar] [CrossRef] [Green Version]
  51. Meneghetti, M.C.Z.; Hughes, A.J.; Rudd, T.R.; Nader, H.B.; Powell, A.K.; Yates, E.A.; Lima, M.A. Heparan sulfate and heparin interactions with proteins. J. R. Soc. Interface 2015, 12, 20150589. [Google Scholar] [CrossRef] [Green Version]
  52. Brusilovsky, M.; Radinsky, O.; Cohen, L.; Yossef, R.; Shemesh, A.; Braiman, A.; Mandelboim, O.; Campbell, K.S.; Porgador, A. Regulation of natural cytotoxicity receptors by heparan sulfate proteoglycans in -cis: A lesson from NKp44. Eur. J. Immunol. 2015, 45, 1180–1191. [Google Scholar] [CrossRef] [PubMed] [Green Version]
Jcm 09 02666 g001 550
Figure 1. Heparin reduced the number of melanoma lung metastases. (A) C57BL/6 mice were injected intravenously with 2 × 105 B16-F10 melanoma cells and treated with heparin (10 mg/kg every 2 days, subcutaneously), starting 1 day after tumor inoculation. After 15 days, mice were euthanized, and lung metastases were macroscopically counted. Graph is representative of two independent experiments. (B) Rag2−/−γc−/− recipients were injected intravenously with 1 × 105 B16-F10, inoculated with 4 × 105 sorted WT or Ncr1−/−(NKp46-deficient NK cells) 12 h later, and treated with heparin as in A. An unpaired t-test was used to compare differences between groups, where * p < 0.05 was used to compare to control.
Figure 1. Heparin reduced the number of melanoma lung metastases. (A) C57BL/6 mice were injected intravenously with 2 × 105 B16-F10 melanoma cells and treated with heparin (10 mg/kg every 2 days, subcutaneously), starting 1 day after tumor inoculation. After 15 days, mice were euthanized, and lung metastases were macroscopically counted. Graph is representative of two independent experiments. (B) Rag2−/−γc−/− recipients were injected intravenously with 1 × 105 B16-F10, inoculated with 4 × 105 sorted WT or Ncr1−/−(NKp46-deficient NK cells) 12 h later, and treated with heparin as in A. An unpaired t-test was used to compare differences between groups, where * p < 0.05 was used to compare to control.
Jcm 09 02666 g001
Jcm 09 02666 g002 550
Figure 2. Heparin stimulates murine NK cells survival, but not proliferation in vitro. NK cells were stained with CellTrace violet (CTV) and plated in 96-well plates in the presence of 50 ng/mL rIL-15 and 100 µg/mL heparin and evaluated by flow cytometry every 24 h. The number of divisions (A), and total cohort (B) were analyzed. Data of three technical replicates of one representative independent experiment out of three. Data are presented as mean ± SEM. Two-way ANOVA was used to compare differences between groups, where * p < 0.05 was considered for statistical significance.
Figure 2. Heparin stimulates murine NK cells survival, but not proliferation in vitro. NK cells were stained with CellTrace violet (CTV) and plated in 96-well plates in the presence of 50 ng/mL rIL-15 and 100 µg/mL heparin and evaluated by flow cytometry every 24 h. The number of divisions (A), and total cohort (B) were analyzed. Data of three technical replicates of one representative independent experiment out of three. Data are presented as mean ± SEM. Two-way ANOVA was used to compare differences between groups, where * p < 0.05 was considered for statistical significance.
Jcm 09 02666 g002
Jcm 09 02666 g003 550
Figure 3. Heparin does not increase the killing capacity of NK cells. (A,B) NK cells isolated from C57BL/6 mice were cultured in the presence of 20 ng/mL of rIL-15 and heparin (10 or 100 µg/mL). After 24 h, NK cells were incubated for 4 h with previously Calcein AM-stained B16-F10 (A) or YAC-1 cells (B). Killing quantification was determined by the intensity of fluorescence in the supernatant and compared to control of each experiment. Each symbol in the scatterplots represents the average of three biological replicates (presented as mean ± SEM). Two-way ANOVA was used to compare differences between groups. (C) NK cells isolated from human peripheral blood mononuclear cells were cultured in the presence of rIL-15 (50 ng/mL), with or without heparin (1 or 100 µg/mL). After 24 h, NK cells were labeled with CTV and co-cultured with A375 cells (ratio 4:1—NK:A375 cell). After 4 h, cells were stained with Annexin V-Fluorescein isothiocyanate (FITC) and propidium iodide and evaluated by flow cytometry. Dead tumor cells were considered CTV-, Annexin V+, and/or PI+. Each point represents technical replicates from two independent experiments (represented by full and empty symbols; presented as mean ± SEM). An unpaired t-test was used to compare differences between groups, with p < 0.05.
Figure 3. Heparin does not increase the killing capacity of NK cells. (A,B) NK cells isolated from C57BL/6 mice were cultured in the presence of 20 ng/mL of rIL-15 and heparin (10 or 100 µg/mL). After 24 h, NK cells were incubated for 4 h with previously Calcein AM-stained B16-F10 (A) or YAC-1 cells (B). Killing quantification was determined by the intensity of fluorescence in the supernatant and compared to control of each experiment. Each symbol in the scatterplots represents the average of three biological replicates (presented as mean ± SEM). Two-way ANOVA was used to compare differences between groups. (C) NK cells isolated from human peripheral blood mononuclear cells were cultured in the presence of rIL-15 (50 ng/mL), with or without heparin (1 or 100 µg/mL). After 24 h, NK cells were labeled with CTV and co-cultured with A375 cells (ratio 4:1—NK:A375 cell). After 4 h, cells were stained with Annexin V-Fluorescein isothiocyanate (FITC) and propidium iodide and evaluated by flow cytometry. Dead tumor cells were considered CTV-, Annexin V+, and/or PI+. Each point represents technical replicates from two independent experiments (represented by full and empty symbols; presented as mean ± SEM). An unpaired t-test was used to compare differences between groups, with p < 0.05.
Jcm 09 02666 g003
Jcm 09 02666 g004 550
Figure 4. Heparin further increases IL-12-mediated IFN-γ production by human NK cells. NK cells isolated from umbilical cord blood were cultured in the presence of rIL-15 (50 ng/mL) and rIL-18 (50 ng/mL), with or without heparin (1 or 100 µg/mL) or rIL-12 (10 pg/mL) for 24 h. The supernatant was collected and IFN-γ quantified by ELISA. Each point represents technical replicates from two independent experiments (represented by full and empty symbols; presented as mean ± SEM). An unpaired t-test was used to compare differences between groups, where * p < 0.05 was used to compare to control.
Figure 4. Heparin further increases IL-12-mediated IFN-γ production by human NK cells. NK cells isolated from umbilical cord blood were cultured in the presence of rIL-15 (50 ng/mL) and rIL-18 (50 ng/mL), with or without heparin (1 or 100 µg/mL) or rIL-12 (10 pg/mL) for 24 h. The supernatant was collected and IFN-γ quantified by ELISA. Each point represents technical replicates from two independent experiments (represented by full and empty symbols; presented as mean ± SEM). An unpaired t-test was used to compare differences between groups, where * p < 0.05 was used to compare to control.
Jcm 09 02666 g004

Share and Cite

MDPI and ACS Style

Rossi, G.R.; Gonçalves, J.P.; McCulloch, T.; Delconte, R.B.; Hennessy, R.J.; Huntington, N.D.; Trindade, E.S.; Souza-Fonseca-Guimaraes, F. The Antitumor Effect of Heparin is not Mediated by Direct NK Cell Activation. J. Clin. Med. 2020, 9, 2666. https://doi.org/10.3390/jcm9082666

AMA Style

Rossi GR, Gonçalves JP, McCulloch T, Delconte RB, Hennessy RJ, Huntington ND, Trindade ES, Souza-Fonseca-Guimaraes F. The Antitumor Effect of Heparin is not Mediated by Direct NK Cell Activation. Journal of Clinical Medicine. 2020; 9(8):2666. https://doi.org/10.3390/jcm9082666

Chicago/Turabian Style

Rossi, Gustavo R., Jenifer P. Gonçalves, Timothy McCulloch, Rebecca B. Delconte, Robert J. Hennessy, Nicholas D. Huntington, Edvaldo S. Trindade, and Fernando Souza-Fonseca-Guimaraes. 2020. "The Antitumor Effect of Heparin is not Mediated by Direct NK Cell Activation" Journal of Clinical Medicine 9, no. 8: 2666. https://doi.org/10.3390/jcm9082666

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop