Background
Tumor-associated blood vessels exhibit prominent structural and functional abnormalities [
1,
2]. The impaired and abnormal vasculature creates a tumor-promoting hypoxic microenvironment that promotes tumor progression, metastasis, and poor drug delivery [
3,
4]. Conventional approaches have focused primarily on the inhibition of angiogenesis to starve cancerous cells [
5,
6]. These agents primarily target vascular endothelial growth factor (VEGF) and its receptor, VEGFR2 [
5,
6], resulting in an initial reduction of the existing tumor vessels. However, these treatments eventually aggravate hypoxia within the tumor core, triggering other proangiogenic signaling pathways that lead to increased tumor proliferation and metastasis [
7,
8]. To avoid the side effects of conventional therapeutics, remodeling the tumor vasculature is a new approach that has been suggested to be an effective treatment strategy. Normalization of the tumor vasculature delivers increased anticancer benefits. These include efficient drug delivery, infiltration of immune cells by reducing the heterogeneity of intratumoral blood flow, and increased vascular permeability caused by tight associations between endothelial cells and perivascular cells [
9,
10].
Recently, we introduced anti-inflammatory nanoparticles into the vasculature which utilize activated protein C (APC) [
11]. The cytoprotective and anti-inflammatory activity of APC is mediated through binding to its receptor, endothelial cell protein C receptor (EPCR). This occurs through the
γ-carboxyglutamic acid (Gla) domain and results in simultaneous activation of protease-activated receptor-1 (PAR-1) signaling via the thrombin receptor agonist peptide (TRAP) domain [
12,
13]. APC also exhibits anti-coagulation activity. While the antithrombotic activity of APC is based on its ability to inactivate clotting factors Va and VIIIa, leading to adverse bleeding, the cytoprotective effect is based on its anti-inflammatory, antiapoptotic, and endothelial barrier stabilization activities [
12,
14].
Since the activation of PAR-1 signaling by TRAP mimics thrombin activity [
15] and results in a cytoprotective response when EPCR is occupied with APCs [
15,
16], both the PC-Gla and TRAP peptides were attached to the surface of ferritin nanoparticles [
11]. Ferritin nanoparticles are useful biocompatible, biodegradable, and nontoxic platforms compared with synthetic polymers [
17], and ferritin-binding sites and ferritin internalization have been identified in some tumor cells [
18]. Therefore, we used small ferritin as a basic template to create nanoparticles [
11]. The PCNs consist of both EPCR-targeting peptides (PC-Gla) and PAR-1-activating peptides (TRAP) on their surface. A TRAP-small ferritin (sFn)-PC-Gla (TFG) or a matrix metalloproteinase (MMP)-2 cleavage site is inserted between sFn and the PC-Gla domain (TFMG). As MMP-2 is overexpressed in inflammatory sites as well as in the tumor microenvironment [
19], PC-Gla is released upon reaching MMP-2 activating sites. Free PC-Gla will not likely interfere with the remaining TRAP-ferritin during the simultaneous double binding to each receptor by the TFMG nanoparticle [
11]. Therefore, these ferritin-based protein cage protein C nanoparticles (PCNs) have simultaneous double occupancy of EPCR and PAR-1, but lack the ability to degrade procoagulant co-factors. Thus, they exhibit high therapeutic efficacy without causing bleeding complications [
11]. Since cancer therapeutic research using nanoparticles to target the tumor vasculature has not been largely explored, we investigated the antitumor activity of PCNs through a new approach which results in the inhibition of tumor progression and metastasis.
In the present study, we used Lewis lung carcinoma (LLC) allograft and MMTV-PyMT spontaneous breast cancer models to demonstrate that PCNs exhibit antitumor and anti-metastatic activity. We found that the PCNs remodeled tumor vessels by increased pericyte coverage and led to improved tumor permeability, increased cisplatin cytotoxicity, and induced normalization of the tumor vasculature. In addition, we found that the PCNs significantly decreased the hypoxic area while increasing blood perfusion of tumor vessels by activating EPCR/PAR-1 and Tie2 simultaneously. This ameliorated the immune response as evidenced by increased antitumor T cell infiltration and decreased M2-like tumor-associated macrophages (TAM). Thus, our studies provide a foundation for the development of therapeutic strategies using nanoparticles that target tumor vascular normalization with antiseptic activity.
Methods
Materials
Bevacizumab was purchased from (InvivoGen, California, USA) and cisplatin (cis-diammineplatinum (II) dichloride, Cis), isopropyl-β-d-1-thiogalactopyranoside (IPTG), imidazole, and dithiothreitol (DTT) were purchased from Sigma-Aldrich (St Louis, MO, USA). Tris-HCl and Triton X-100 were purchased from Amresco (Solon, OH, USA), sodium chloride and urea from Junsei Chemical (Tokyo, Japan), and phenylmethane sulfonyl fluoride (PMSF) and protease inhibitor cocktail tablets from Roche (Basel, Switzerland). Mouse monoclonal antibodies against α-smooth muscle actin (SMA), pimonidazole, and cytokeratin II were purchased from Abcam (Cambridge, UK), HPI (Burlington, MA, USA), and Millipore (Burlington, CA, USA), respectively. Antibodies against CD31 and LYVE-1 were obtained from BD Biosciences (San Jose, CA, USA) and Angiobio (San Diego, CA, USA), respectively. Alexa Fluor 488-, 568-, and 647-conjugated antirabbit IgG and Hoechst 33258 were obtained from Invitrogen (Carlsbad, CA, USA).
Expression and purification of the PCNs
The TFG/TFMG vectors were constructed, expressed, and purified as previously reported [
11]. Briefly, TFG/TFMG plasmids were transformed into
Escherichia coli expression strain BL21 (DE3) and grown in LB medium containing 50 μg/ml kanamycin. Protein expression was induced with 0.1 M IPTG at 37 °C for 5 h, and the cells were lysed (lysis buffer: 50 mM Tris-HCl pH 6.8, 100 mM NaCl, 1% Triton X-100, 1 mM PMSF, 1 mM DTT, protease inhibitor cocktail) and ultrasonicated. Binding was performed (urea binding buffer: 20 mM Tris-HCl pH 6.8, 300 mM NaCl, 10 mM imidazole, 8 M urea) at room temperature for 1 h. The sample was loaded onto nickel ion chelate affinity columns, washed (washing buffer: 20 mM Tris-HCl pH 6.8, 500 mM NaCl, 30 mM imidazole, 8 M urea), and eluted (elution buffer: 20 mM Tris-HCl pH 6.8, 100 mM NaCl, 300 mM imidazole, 8 M urea). Finally, sequential dialysis (dialysis buffer: 20 mM Tris-HCl pH 6.8, 100 mM NaCl, and sequentially diminishing concentration of urea) using a dialysis cassette (MWCO, 10 kDa; Thermo Scientific, Rockford, IL, USA) was conducted to obtain refolded proteins.
Protein gel staining
SDS-PAGE gel staining assay was performed to evaluate the purity of TFG and TFMG following protein purification. First, the protein samples were separated by gel electrophoresis using a 10% SDS-PAGE gel, followed by washing and visualization of the protein bands by staining with a solution containing Coomassie brilliant blue R250 dye (0.125 g), glacial acetic acid (5 ml), methanol (25 ml), and water (20 ml), followed by destaining. Photographic images of the gels were captured to record the protein bands.
Cell culture
LLC and EA.hy926 (human endothelial somatic cell hybrid) cells were obtained from the American Type Culture Collection (Manassas, VA, USA), and C3H/10T1/2 (clone 8) cells were obtained from the Korean Cell Line Bank (Seoul, South Korea). All of the cells were grown in DMEM (Hyclone, Logan, UT, USA) supplemented with 10% FBS (Hyclone, Logan, UT, USA) and 1% antibiotics (100 units/ml penicillin, 100 mg/ml streptomycin, and 0.25 mg/ml amphotericin B; Invitrogen, Carlsbad, CA, USA) at 37 °C in a humidified atmosphere containing 5% CO2 and 95% air.
Mice
The mice used in this study consisted of 5- to 6-week-old adult male C57BL/6J mice (SLC, Japan) or
MMTV-
PyMT transgenic mice [
20,
21] (Jackson Lab, Sacramento, CA, USA). All mice were housed in a specific pathogen-free facility with individual ventilation systems at Kyungpook National University. The animal handling and experimental procedures were conducted strictly according to the Guidelines for Care and Use of Laboratory Animals issued by the Institutional Ethical Animal Care Committee of Kyungpook National University (Protocol number: KNU 2014-0189 and KNU 2017-0145).
Pharmacokinetic study
After intravenous injection of TRAP (10 nmol/kg) into the tail vein of mice, plasma samples (30 μl) were obtained at 0.5, 1, 1.5, and 2 h. Plasma samples (30 μl) were vigorously mixed with 100 μl acetonitrile and centrifuged at 16,000 g for 10 min. Aliquots (20 μl) of the supernatant were injected into an Agilent 6470 Triple Quadrupole mass spectrometer equipped with an Agilent infinity 1260 high-performance liquid chromatograph (Agilent, Wilmington, DE, USA). TRAP was monitored using multiple reaction modes at m/z 761.6 → 602.5 in the ionization mode with a collision energy of 35 eV. After intravenous injection with DyLight 680 NHS ester-conjugated TFMG (10 nmol/kg) into the tail vein of LLC allograft tumor-bearing mice, plasma samples (30 μl) were obtained at 0.5, 2, 4, 8, 24, and 48 h. The fluorescence of the TFMG in plasma samples was measured at excitation and emission wavelengths of 685 nm and 715 nm, respectively. The calibration standards for TRAP and TFMG in mouse plasma were linear in the range of 0.28–72 nM with a correlation coefficient of over 0.999. The pharmacokinetic parameters were calculated using the non-compartmental model in WinNonlin (version 5.1; Pharsights, Cary, NC, USA).
Development of tumor models and treatment regimens
To generate a LLC allograft tumor model, suspensions of LLC cells (4 × 105 cells in 200 μl of serum-free culture media) were implanted subcutaneously into the dorsal flank regions of 5- to 6-week-old male C57BL/6J mice. At the indicated time points following LLC cells inoculation, the mice were administered TFG (10 nmol/kg) or TFMG (10 nmol/kg), with or without cisplatin (3 mg/kg), or bevacizumab (5 mg/kg) by intravenous injection into the tail vein. Subsequently, tumor volumes were measured based on the formula: V = 0.5 × A × B2, where A represents the longest and B the shortest dimension. Eventually, the mice were anesthetized and tissues were harvested for further analyses at the completion of the study period.
Female MMTV-PyMT transgenic mice were employed as another model to observe tumor growth and metastasis. Twelve weeks following their birth, the volumes of every palpable tumor nodule were measured and added to determine the tumor burden for each mouse. Based on tumor burden, the mice were divided into three groups, each receiving TFG (10 nmol/kg), TFMG (10 nmol/kg), or vehicle (control) at the indicated time points. Tumor burdens after each week following the 12th week were measured up to the 15th week for each of the three groups. At the 15th week, the mice were anesthetized and tissues were harvested for further analyses.
Immunohistochemical and histological analyses
For immunohistochemical (IHC) analysis, the harvested tumor or tissue samples were fixed in 3.7% formaldehyde (FA), dehydrated by serially incubating with 10% to 40% sucrose solution, and finally embedded in tissue freezing medium (Leica, Wetzlar, Germany). The frozen blocks were cut into 5 to 10 μm sample sections, which were blocked with 5% BSA in PBST (0.3% Triton X-100 in phosphate-buffered saline (PBS)) and incubated overnight at 4 °C with the appropriate primary antibody: anti-CD31 (BD Biosciences, CA, USA), anti-CD31 (Milipore, MA, USA), anti-α-SMA (Abcam, Cambridge, UK), antipimonidazole (Hypoxyprobe-1, HPI, MA, USA), anticytokeratin II (Millipore, MA, USA), anti-LYVE-1 (Angiobio, CA, USA), anti-Phospho-Tie-2 (R&D systems, MN, USA), anti-PAR1 (Abcam, Cambridge, UK), anti-PAR3 (Santa Cruz, CA, USA), anti-CD68 (Abcam, Cambridge, UK), anti-iNOS (Abcam, Cambridge, UK), anti-arginase1 (BD Biosciences, CA, USA), anti-CD4, PE (Invitrogen, CA, USA), or Alexa Fluor 647 anti-CD8a (BioLegend, CA, USA). After a few washes, the samples were incubated at RT for 1 h with the recommended fluorophore-tagged secondary antibody, their nuclei stained with Antifade Mounting Medium with DAPI (Vector Laboratories, Burlingame, CA) or Hoechst 33258 (Invitrogen, USA), and mounted with fluorescent mounting medium (Sigma, USA). The immunofluorescence images were acquired using a Leica TCS SP5 II confocal microscope (Leica, Wetzlar, Germany) or a Zeiss confocal microscope (Carl Zeiss, Germany). Pimonidazole hydrochloride (60 mg/kg; Hypoxyprobe-1, HPI, USA) was injected intraperitoneally 90 min before sacrifice of mice bearing tumors used for the investigation of hypoxic regions. Serial tissue sections (5 μm) were stained with H&E and observed under an Axio Imager A1 light microscope (Carl Zeiss, Germany).
Terminal deoxynucleotidyl transferase-mediated dUTP nick-end green fluorescent labeling assay
Tumor tissues were fixed with 4% paraformaldehyde in PBS at 4 °C for 24 h and frozen sections were prepared. The terminal deoxynucleotidyl transferase-mediated dUTP nick-end green fluorescent labeling (TUNEL) assay was performed with sectioned tissues (5–10 μm thickness) according to the manufacturer’s instructions (TUNEL assay kit, Promega, Madison, WI, USA). Fluorescent images were observed by fluorescence microscopy (Axio Imager A1 microscope Carl Zeiss, Germany).
In vivo vascular leakage and perfusion assays
On the day of the last PCN injection, a vascular perfusion assay was performed by injecting 100 μl of DyLight® 488-labeled Lycopersicon esculentum (tomato) lectin (1 mg/ml, Vector Lab) intravenously 30 min prior to sacrifice. To check for vascular leakage, 100 μl of FITC-dextran (25 mg/ml, 70 kDa, Sigma-Aldrich) was intravenously injected into the mice 30 min before sacrifice. After the mice were perfused with PBS and 4% paraformaldehyde (PFA), the FITC-dextran or tomato-lectin in the tumor tissues were observed under a Leica TCS SP5 II Dichroic/CS confocal microscope (Leica, Wetzlar, Germany). The fluorescence intensity was measured using ImageJ software.
Conjugation of fluorophores to TFMG
TFMG was labeled with Dylight 680 NHS ester at a molar ratio of 1:10. Briefly, TFMG (1 mg) was dissolved in PBS (1.5 ml) and Dylight 680 NHS ester (1 mg) was dissolved in DMSO (0.1 ml). TFMG and fluorescent dye were incubated for 2 h at room temperature. The reaction product was passed through a 0.2-μm filter unit, and the unreacted dye was separated on a PD midiTrap™ G-25 (GE Healthcare, UK) column that had been pre-equilibrated with PBS and 2 mM sodium azide. This process yielded 300 μM of TFMG with a ratio of dye per protein greater than 1.5.
In vivo imaging for biodistribution
The animal study was conducted using the same protocol described above. A total of 8 C57BL/6J mice were randomized and grouped. Two mice were allocated to receive non-labeled TFMG treatment (control). For the TFMG-treated group, 6 mice were divided into 2 time points (n = 3): 3 and 6 h. TFMG was diluted in saline and administered intravenously once at an equivalent dose of 5.48 μg/mouse via the tail vein. The animals were imaged by IVIS® Spectrum CT (Perkin Elmer, Waltham, MA).
Gene silencing and quantitative real-time polymerase chain reaction
EA.hy926 and C3H/10T1/2 cells were transfected with 10 to 200 nM of siRNA for
PAR-
1,
PAR-
2,
PAR-
3,
Tie2,
Gα13,
Gαi, or
Gαq (Bioneer, Daejeon, South Korea) using Lipofecatmine RNAiMAX. Silencing of the genes was confirmed by quantitative real-time polymerase chain reaction (qRT-PCR) using the primers shown in Table
S2. After total RNA was extracted using a Trizol RNA extraction kit (Invitrogen, California, USA), cDNA was reverse-transcribed using ReverTra Ace® qPCR RT Master Mix (TOYOBO, Osaka, Japan). Quantitative real-time PCR was performed with SsoAdvanced Universal SYBR® Green Supermix (Bio-rad, Hecules, CA, USA) (Bio-rad C1000 Thermocycler). Relative expression to β-actin was calculated by the ΔΔCt method (Livak and Schmittgen 2001).
In vitro cell co-cultures
Endothelial cell/cancer cell (EC) co-cultures, pericyte/cancer cell (PC) co-cultures, and pericyte/endothelial cell/cancer cell (PEC) co-cultures were established using EA.hy926, LLC, and C3H/10T1/2 cells. For the EC co-cultures, LLC cells (2.5 × 105 cells/well) were first seeded in 12-well plates and allowed to adhere for 4 h, after which 12-well Transwell polycarbonate membrane inserts (3 μm; Corning, NY, USA) were placed above each well. EA.hy926 cells (5 × 105 cells/well) were seeded over the Transwell membrane inserts and incubated at 37 °C for 48 h. For PC co-cultures, LLC (2.5 × 105 cells/ well) cells were seeded onto the 12-well plate surface, while C3H/10T1/2 cells (2.5 × 105 cells/well) were seeded above the Transwell membrane inserts. For the PEC co-cultures, LLC (2.5 × 105 cells/ well) cells were seeded onto the 12-well plate surface, and C3H/10T1/2 cells (2.5 × 105 cells/well) were added to the lower surface of the Transwell membrane inserts and was followed by the addition of EA.hy926 cells (5 × 105 cells per well) onto the upper surface of the Transwell membrane inserts. The other procedures remained the same.
In vitro cell permeability analysis
EC, PC, and PEC co-cultures were used to conduct permeability assays. The EC, PC, and PEC co-cultures were treated with TFG or TFMG and incubated at 37 °C for 24 h. Transwell membrane inserts were washed with PBS and transferred to fresh 12-well plates containing 500 μl of serum-free DMEM per well. FITC-dextran (150 μl; 50 μg/ml; MW = 3 kDa; Sigma-Aldrich, MO, USA) was added to each of the Transwell membrane inserts, and leakage across the Transwell membrane was determined using a fluorescence plate reader (λex, 485 nm; λem, 535 nm).
Immunoprecipitation
EA.hy926 cells (1 × 106) were seeded in 100 mm cell culture plates, incubated overnight at 37 °C, and treated with 100 nM TFG or TFMG for 24 h. The cells were then washed with PBS, detached, and lysed with RIPA buffer solution. An appropriate amount of protein was mixed with anti-PAR-3 antibody and incubated overnight at 4 °C under constant rotation. Magnetic beads were added and the mixture was rotated at 4 °C for 4 h to permit binding. After washing and eluting, immunoblots were recorded to visualize the co-immunoprecipitated proteins.
Western blot analysis
EA.hy926 cells were seeded into 6-well plates, incubated overnight at 37 °C, and treated with 100 nM TFG or TFMG for a suitable duration. The cells were then washed with PBS, detached, and lysed with RIPA buffer solution. Equal amounts of proteins were separated using SDS-PAGE gels and transferred to PVDF membranes. After blocking, the membranes were incubated with antibodies against p-Tie2 (1:1000), Tie2 (1:200), p-Akt (1:1000), Akt (1:1000), FoxO1 (1:1000), p-FoxO3a (1:1000), FoxO3a (1:1000), ROCK-1 (1:1000), ZO-1 (1:1000), or β-actin (1:5000) at 4 °C for 12 h. Membranes were washed three times for 10 min and incubated with a 1:3000 dilution of anti-mouse, anti-goat, or antirabbit antibodies for 2 h. The Western blots were visualized by chemiluminescent detection.
Immunofluorescence
EA.hy926 cells (2 × 105 cells/well) were seeded onto glass coverslips in 4-well plates, incubated overnight at 37 °C, and treated with 100 nM TFMG for 24 h. The cells were then washed with PBS, fixed with 3.7% formaldehyde (Sigma-Aldrich, St Louis, MO, USA), and permeabilized with 0.1% Triton X-100 (Amresco, Solon, OH, USA). After 1 h of blocking with 3% BSA, the cells were incubated overnight at 4 °C with the required primary antibody solution in 0.1% BSA. After washing with PBS the following day, the cells were incubated at room temperature for 1 h with the appropriate fluorescence-tagged secondary antibody solution in 0.1% BSA. The coverslips were mounted onto glass slides using mounting gel and the images were visualized and recorded using a Leica TCS SP5 II confocal microscope (Leica, Wetzlar, Germany).
Statistical analysis
Statistical analysis was carried out using Graph Pad Prism 7.0. Significant differences for individual pairs of means were determined using Student’s
t test and for lager datasets comparing more than 3 groups, one-way ANOVA was used followed by post hoc Dunnett’s multiple comparison test where appropriate to analyze the level of significance, with
p values < 0.05 considered statistically significant. Two-way ANOVA was used when there is more than one independent variable and multiple observation for the mean differences between groups. All the data were expressed as means ± standard deviation (SD) of at least 3 replicates. For the analysis of synergism of combination therapy, the Bliss independence model was utilized [
22]. The expected response tumor volume (
VExp) for the combination groups was defined by the formula:
VExp = (
V1 ×
V2)/
VC, where
V1 and
V2 are the mean tumor volumes in the single-treatment group and
VC is the mean volume in the control group. The tumor volume change from the baseline of control group was defined as Δ
V =
VC −
V0 (initial volume). Then, the range around the
VExp was calculated, via upper (
U) and lower (
L) limits, as follows:
VExpU =
VExp + 0.15 × Δ
V and
VExpL =
VExp − 0.15 × Δ
V. If
VObs is less than
VExpL, it indicates a synergistic effect, and if
VObs is in-between
VExpL and V
ExpU, it denotes an additive effect.
VObs: the observed mean tumor volume in the combination groups.
Discussion
Tumors are not properly perfused due to destabilization of vascular structure and increased interstitial fluid pressure, which result in extreme hypoxia and impaired drug delivery. These alterations, in turn, enhance tumor progression, tissue invasion, metastasis, and resistance to chemotherapy [
1]. Tumor vascular normalization, which is aimed at increasing perfusion and oxygenation, is associated with better clinical responses in subsets of diverse cancer patients [
2]. In the present study, we demonstrated that ferritin-based protein C nanoparticles exhibited antitumor and anti-metastatic effects through tumor vascular normalization and antitumorigenic immune reprogramming in mouse models. The PCNs, TFG and TFMG, induced tumor vascular normalization by PAR-1/PAR-3 heterodimerization and Tie2 activation, which stabilized the vascular tight junctions through the Akt-FoxO3a signaling axis. The PCNs increased the number of cytotoxic CD8
+ T lymphocytes and CD68
+iNOS
+ M1-like macrophages, induced minimal changes in CD4
+ T lymphocytes, and decreased CD68
+/Arg-1
+ M2-like macrophages in tumor tissues. In addition, PCNs enhanced the chemotherapeutic effects of cisplatin by increasing blood perfusion and decreasing vascular permeability. These results suggest that the PCNs represent an efficient antiangiogenic therapeutic option to avoid the side effects of conventional angiogenic therapy or chemotherapy for treatment of advanced solid tumors.
The PCNs induced a significant inhibition of tumor growth both in an LLC mouse model and a spontaneous
MMTV-
PyMT breast tumor model, increased pericyte coverage, and reduced hypoxia in tumor sections. Vascular permeability drives (or vice versa) tumor-induced angiogenesis, inflammatory cell infiltration, and tumor extravasation, which ultimately increases metastatic potential [
3,
4]. Hence, tumors strive to overcome the microenvironmental stress of vascular permeability in order to alleviate excessive angiogenesis and tumor extravasation [
24]. Interestingly, increased blood flow into the tumor by normalization provides sufficient oxygen supply and increased drug delivery resulting in cancer cell death by immune cell penetration [
10,
21]. Hypoxic areas in xenograft or metastatic tumors were reduced by TFG/TFMG treatment in mouse models, suggesting that vascular permeability is decreased while perfusion is increased by the PCNs.
Hypoxia causes immunosuppression by recruiting and activating immune suppressor cells such as regulatory T (Treg) cells and TAM cells [
24]. The PCNs promoted an increased infiltration of cytotoxic T cells, but decreased regulatory T cells. The polarization of TAM and T cell infiltration by the PCNs may be induced by the disappearance of hypoxic regions in tumor tissues. Since an abnormal vasculature is advantageous for elevated hypoxia, defective immune cell trafficking, and tumor malignancy [
10], our new therapeutic approach for converting the abnormal vasculature to a normal vasculature using PCNs is a powerful treatment option for advanced solid tumors.
EPCR binding activity is obtained by the Gla domain and PAR-1 cleavage activity is obtained by the TRAP domain of the PCNs. After cleavage of extracellular PAR-1 at the R46 residue [
46], heterodimerization of PAR-1 with PAR-3 may occur, leading to Tie2 recruitment and activation. Here, we demonstrated that PCNs simultaneous occupy EPCR and activates the Tie2 receptor resulting in endothelial tight junctions. TFMG-induced inhibition of in vitro permeability in EC co-cultures was effectively antagonized by siRNA-mediated endothelial Tie2 silencing as well as antibody-mediated endothelial Tie2 blockage, which is implicated in Tie2 activation. This further led to increased levels of tight-junction marker proteins in the endothelial cells. As Tie2 activation has been shown to be an important event in the normalization of tumor vessels [
21] as well as in sepsis [
47], targeting EPCR and Tie2 by PCNs represents a highly efficient and effective way to treat cancers.
To further identify the signaling pathway underlying PCN antitumor activity, we investigated the EPCR/Tie2-mediated signaling pathway in endothelial cells. G
α13 G-protein is involved in the activation of RhoGTPase nucleotide exchange factors (RhoGEFs), the downstream target of PAR-1/PAR-3, which leads to activation of the small monomeric GTPase, RhoA, and other downstream effectors [
48]. In addition, Akt promotes endothelial barrier protection through a FoxO-mediated pathway, regulating turnover of tight-junction proteins, such as ZO-1 [
49]. The PCN-activated G
α13/RhoA may phosphorylate Tie2 and induce the activation of Akt and FoxO3a, resulting in an enhancement of tight junctions by increasing ZO-1 (Fig.
6e). These results suggest that the Tie2/Akt/FoxO3a signaling axis mediated through PAR-1/PAR-3 heterodimerization is an essential signaling pathway for the normalization of tumor vessels by the PCNs.
Excellent clinical results have been commonly associated with nanoparticle drug delivery systems exhibiting high clinical efficacy and significantly reduced adverse effects [
50,
51]. Ferritin nanoparticles are useful platforms for therapeutic agents. They can be chemically modified to impart functionalities within their interior cavities or on their surfaces because of their unique architecture [
17]. Unlike most other proteins, ferritin possesses unique properties, such as high solubility, stability, abundance in blood, and low toxicity, which motivates studies on its use as an ideal nanoplatform with many applications including disease therapy and drug delivery [
18]. Here, we used ferritin as a template to encapsulate and deliver PCNs as a potential cancer therapeutic. In addition, we showed that concomitant administration of cisplatin with PCNs significantly enhanced antitumor activity and survival because of the capability of PCNs to normalize abnormal tumor vessels. If anticancer drugs can be used at lower doses while maintaining efficient delivery, reduced side effects would be expected [
52]. Therefore, combination therapy using anticancer drugs with the PCNs may be an excellent therapeutic strategy.
In the present study, we showed that PCNs could be used to enhance normalization of the tumor vasculature and increase the immune response in the tumor microenvironment. The underlying mechanisms involved in PCN-induced vascular normalization involve endothelial PAR-3 and Tie2 activity following EPCR binding and PAR-1 activation. PAR-1 activation by the PCNs led to PAR-1/PAR-3 heterodimerization, which subsequently induced activation of the Gα13-RhoA GTPase and Tie2 signaling. This ultimately resulted in increased recruitment of tight-junction proteins through FoxO3-mediated transcription at endothelial cell junctions. In addition, PCN-induced Tie-2 activation promotes pericyte coverage of the tumor vasculature and hypoxic regions even at core regions of the tumor.
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