Application of tumor pH/hypoxia-responsive nanoparticles for combined photodynamic therapy and hypoxia-activated chemotherapy

Introduction

In recent years, a variety of nanocarriers has been designed to deliver therapeutic agents for combined chemo-photodynamic therapy (chemo-PDT) (Kim et al., 2017; Pei et al., 2019; Yu et al., 2023). The complementary cell-killing mechanisms of combined chemo-PDT eliminate the limitations of monotherapy and improve anticancer therapeutic efficacy (Conte et al., 2016; Cheng et al., 2020; Majerník et al., 2022). Despite the theoretical promise of chemo-PDT, outcomes are significantly limited by a lack of precise tumor targeting. Rather than relying on passive enrichment in tumors via enhanced permeability and retention (EPR), tethering cell-penetrating peptides (CPPs) to the nanocarriers promotes payload delivery to tumor cells (Guidotti et al., 2017; Zorko et al., 2022). However, the clearance by macrophages and non-specific distribution in healthy tissue are major obstacles that limit the efficacy of CPPs (Deshpande et al., 2013; Futaki and Nakase, 2017). To overcome these limitations, CPP function must be precisely masked in the bloodstream and activated only within the targeted solid tumors (Dohmen and Wagner., 2011; Zhu et al., 2013). Many studies have focused on developing strategies for spatially controlled, tumor-specific CPP presentation (Huang et al., 2013; Li et al., 2014; Ruoslahti, 2017; Jing et al., 2018; Mohammed et al., 2019). Due to its homogeneity and stability, extracellular acidity (pH_e ∼6.5–6.8) is a promising stimulus, and growing evidence has suggested the outstanding sensitivity of the dimethyl maleate (DA) moiety to pH_e (Du et al., 2011; Gao et al., 2017; Ma and Sun, 2020).

The photosensitization reaction generally produces many toxic reactive oxygen species (ROS) by consuming surrounding oxygen (Abrahamse and Hamblin, 2016; Han et al., 2022; Tang et al., 2022). As a result, cells that survive PDT exist in a hypoxic microenvironment, and hypoxia-induced chemoresistance has become a critical issue in these residual cells (Wang et al., 2017; Yang et al., 2021). Hypoxia-inducible factor-1α activity is upregulated, altering metabolism and drug efflux in hypoxic tumor cells (Majmundar et al., 2010; Cairns et al., 2011; Ma et al., 2022). Hypoxia also alters DNA methylation and autophagy, which are related to chemotherapy resistance (Jing et al., 2019; Kopecka et al., 2021). Pioneering studies have demonstrated that hypoxia-activated prodrugs (HAPs), which can be converted from non-toxic to toxic molecules under hypoxic conditions, offer a powerful strategy that can be combined with PDT for the selective killing of hypoxic cells after PDT (Feng et al., 2017; Sun et al., 2019; Zhu et al., 2019; Jiang et al., 2022). HAPs typically interact with nuclear DNA, so boosted intracellular drug release is also a highly desirable feature of nanocarriers (Li et al., 2021; Yang et al., 2022). Specific and effective cancer therapy requires the design of nanosystems with pH_e-sensitive TAT presentation and hypoxia-boosted cargo release to simultaneously achieve tumor homing and HAP liberation and activation inside the targeted tumor.

We developed a mixed polymeric micelle (^DANP_CT) capable of TAT presentation at pH_e and hypoxia-responsive dissociation for controlled PDT and hypoxia-activated chemotherapy. TAT-modified poly (ethylene glycol)-polyphosphoesters (TAT-PEG-PHEP) and 2-nitroimidazole-grafted PEGylated polyphosphoesters PEG-b-P (AEP-g-NI) were self-assembled to encapsulate chlorin e6 (Ce6; photosensitizer) and tirapazamine (TPZ; HAPs). We hypothesized that ^DANP_CT could achieve prolonged blood circulation due to temporary shielding of the TAT ligands via the DA moiety (Figure 1). After entering the tumor matrix, pH_e-induced DA deshielding activated the TAT to promote cellular penetration. PDT with a 660-nm laser triggered the production of cytotoxic ROS, thus leading to cell killing and O₂ consumption. Local hypoxia converted hydrophobic NI to hydrophilic 2-aminoimidazole to facilitate ^DANP_CT dissociation and TPZ release and activation to produce toxic radical species for the selective killing of hypoxic cells that remain after PDT. Cascade-amplified therapeutic outcomes were studied in vitro and in vivo.

FIGURE 1

FIGURE 1. Scheme of ^DANP_CT design and pH_e-sensitive TAT presenting and PDT-induced hypoxia-activated chemotherapy.

Materials and methods

Materials

Ce6, 2,2-dimethoxy-2-phenyl acetophenone (DMPA), and TPZ were obtained from Macklin. We synthesized (2-nitro-1H-imidazol-1-yl) methanethiol (NI-SH), the diblock copolymer of PEG-b-PAEP, and TAT-PEG-PHEP as described previously (Li et al., 2017; Ma and Sun, 2020). The cell counting kit-8 (CCK-8) was obtained from Shanghai Saint-Bio. Dulbecco’s modified Eagle’s medium (DMEM) and fetal bovine serum (FBS) were purchased from Gibco (Gibco, United States). Phalloidin-Alexa Fluor 488 and DAPI were obtained from Beyotime Biotechnology. All other reagents were of analytical grade and used as received.

Synthesis of diblock PEG-b-P (AEP-g-NI)

NI-SH (292.8 mg; 1.84 mmol) and DMPA (14.1 mg) were mixed in THF (16 mL) containing 287.2 mg PEG-b-PAEP and purged with Ar₂ for 25 min. The reaction was incubated for 60 min at room temperature under a 365-nm UV light, then transferred to a dialysis tube (MWCO 3500 Da), and dialyzed against ddH₂O at 4°C. The solution was lyophilized to obtain PEG-b-P (AEP-g-NI).

Preparation of Ce6 and TPZ-loaded nanocarriers

TAT-PEG-PHEP, PEG-b-P (AEP-g-NI), Ce6, and TPZ were mixed at a weight ratio of 3:7:1:1 in DMF. The organic solution was then added slowly to ddH₂O under gentle stirring. After stirring overnight, DMF and unencapsulated Ce6 and TPZ were removed by dialysis against ddH₂O. After centrifugation at 800 g for 15 min, the nanoparticles (NP_CT) were collected. To fabricate pH_e-sensitive ^DANP_CT, NP_CT was reacted with excess 2,3-dimethylmaleic anhydride in ddH₂O at pH 8–9 and 4°C for 6 h and then purified by ultrafiltration. A similar method was used to prepare pH_e-insensitive ^SANP_CT with succinic anhydride instead of 2,3-dimethylmaleic anhydride.

Cellular uptake of nanocarriers at different pH conditions

MCF-7 cells were seeded in 24-well plates and incubated with fresh DMEM containing NP_CT, ^SANP_CT, or ^DANP_CT (pretreated at pH 7.4 or 6.5) at 37°C for 6 h. The cells were washed with cold PBS, fixed with paraformaldehyde, and analyzed by FACS. Total protein and Ce6 concentrations in the cell lysate were analyzed using a bicinchoninic acid kit and spectrofluorimetry, respectively.

MCF-7 cells were seeded on coverslips in 12-well plates and incubated with NP_CT, ^SANP_CT, or ^DANP_CT (pretreated at pH 7.4 or 6.5) at 37°C for 6 h. The cells were washed with PBS, fixed with 4% paraformaldehyde, and then stained with phalloidin-Alexa Fluor 488 and DAPI, according to standard protocols. The cells were then visualized on a Zeiss LSM 810 confocal laser scanning microscope.

Cell killing by ^DATAT-NP_Ce6 in vitro

To study the biocompatibility of nanoparticles that have not been loaded with Ce6 or TPZ, MCF-7 cells were seeded in 96-well plates (10,000 cells per well) and incubated with NP, ^SANP, or ^DANP for 72 h. To study the therapeutic efficacy of PDT and hypoxia-activated chemotherapy, MCF-7 cells were seeded in 96-well plates (10,000 cells per well). The normoxic (21% O₂ pressure) or hypoxic condition (2% O₂ pressure) was generated in a three-gas incubator, while the partial pressure of CO₂ was maintained at 5%. NP_CT, ^SANP_CT, or ^DANP_CT was added at pH 7.4 or 6.5, incubated for 4 h, and then incubated with MCF-7 cells under normoxic conditions at different Ce6 concentrations for 24 h. The medium was replaced with DMEM (10% FBS) without nanoparticles, and then, the cells were exposed to a 660-nm laser (100 mW/cm²; 15 min). After incubation for another 48 h under normoxic or hypoxic conditions, viability was measured using a standard CCK-8 assay.

Pharmacokinetics and biodistribution of ^DANP_CT in vivo

Female BALB/c mice were randomly divided into four groups and treated with free Ce6, NP_CT, ^SANP_CT, or ^DANP_CT via tail vein injection (Ce6 10 mg/kg). At 10 min, 30 min, 1 h, 2 h, 4 h, 8 h, 12 h, 24 h, and 48 h post-injection, blood samples were collected from the retro-orbital plexus. The plasma was obtained by centrifugation, and Ce6 content was quantified by high-performance liquid chromatography (HPLC).

To study the accumulation of ^DANP_CT in the major organs and tumor tissues, 1 × 10⁷ MCF-7 cell suspension (200 μL) was injected into the mammary fat pad of female BALB/c nude mice to develop a tumor model. Mice bearing MCF-7 xenografts were treated with an intravenous (i.v.) injection of free Ce6, NP_CT, ^SANP_CT, or ^DANP_CT (Ce6 10 mg/kg). At 6 h, 12 h, and 24 h, tumor tissues and other organs were excised and homogenized, and Ce6 content was quantified by HPLC.

Antitumor efficacy in vivo

Female MCF-7 tumor-bearing BALB/c nude mice were randomly divided into five groups (n = 6), and, once the tumor volume reached ∼100 mm³, the mice were treated with 0.9% NaCl, free Ce6 + TPZ, NP_CT, ^SANP_CT, or ^DANP_CT (TPZ 5 mg/kg) every week. At 12 h post-injection, the tumor sites were exposed to 660-nm light for 15 min at a power density of 200 mW/cm². Tumor volume (0.5 × length × width²) and body weight were monitored every 3 days. On day 24, blood samples and the major organs were collected for ELISA analysis and hematoxylin and eosin (H&E) staining, respectively.

Results and discussion

Preparation of pH_e- and hypoxia-responsive ^DANP_CT

To prepare hierarchically responsive nanocarriers, TAT-PEG-PHEP and hypoxia-sensitive PEG-PAEP-NI were synthesized as described previously. The efficiency of NI modification was approximately 100% after thiol–ene “click” chemistry, as indicated by ¹H NMR spectroscopy (Supplementary Figure S1). Hydrophobic Ce6 and TPZ were encapsulated with TAT-PEG-PHEP and PEG-b-P (AEP-g-NI) at a 3:7 weight ratio to form the mixed micelle (NP_CT). Finally, 2,3-dimethylmaleic anhydride was introduced to react with the lysine amines of NP_CT to yield nanoparticles with pH_e-responsive TAT reactivation properties (^DANP_CT). For comparison, pH_e-insensitive ^SANP_CT was prepared by decoration with succinic anhydride. The hydrodynamic diameter of NP_CT, ^SANP_CT, and ^DANP_CT was measured by dynamic light scattering and transmission electron microscopy. The various nanoparticles had a diameter of ∼80 nm and a uniform, spherical morphology (Figures 2A,B). According to the UV-vis absorbance at 642 and 698 nm, the encapsulation efficacies of the mixed micelles were 2.31% (Ce6) and 2.69% (TPZ), respectively. The average size of the nanoparticles, regardless of TAT modification, remained unchanged in PBS over 168 h (Supplementary Figure S2), verifying the outstanding colloidal stability provided by the outer PEG layer.

FIGURE 2

FIGURE 2. (A) Size distribution of NP_CT, ^SANP_CT, and ^DANP_CT measured by DLS. (B) TEM observation of NP_CT, ^SANP_CT, and ^DANP_CT. The scale bar is 200 nm. (C) Zeta potential change of NP_CT, ^SANP_CT, and ^DANP_CT at pH 7.4 or 6.5. (D) ROS production indicated by DCFH (E_m = 525 nm) of Ce6-loaded nanoparticles. Vitamin C acts as an ROS scavenger.

As expected, the TAT amine groups are exposed to enable cell penetration following degradation at an acidic tumor pH. We monitored the zeta potential at pH 6.5 or 7.4 and found that NP_CT maintained its original zeta potential at both pH values, comparable to that of TAT-decorated nanocarriers reported elsewhere (Figure 2C) (Li et al., 2017; Zhang et al., 2020). However, the zeta potential of ^DANP_CT increased dramatically from +1.4 mV to +15.1 mV at pH 6.5. Meanwhile, the slight zeta potential elevation of ^DANP_CT at pH 7.4 could be explained as the partial breakage of unstable amide bonds within the DA moieties. With SA modification, ^SANP_CT masked the TAT ligand, and a minimal zeta potential change was observed at both pH levels. The fluorescamine method was used to quantify the exposed amine groups. Compared to the control groups, the DA degradation efficiency of ^DANP_CT reached 85.78% ± 4.65% at pH 6.5 (Supplementary Figure S3), and only 22.36% ± 2.58% of DA moieties broke at neutral pH.

The PDT effect at 660 nm was measured using a 2′,7′-dichlorodihydrofluorescein diacetate probe because it was oxidized by ROS to obtain fluorescent DCFH (Eruslanov and Kusmartsev, 2010; Kim and Xue, 2020). Emission fluorescence measurements of NP_CT, ^SANP_CT, and ^DANP_CT at 525 nm (excitation = 488 nm) revealed comparable laser power-dependent ROS production rates (Figure 2D). The fluorescence intensity of DCFH induced by NP_CT, ^SANP_CT, and ^DANP_CT was reduced by nearly ∼11.6-fold after adding an ROS scavenger (vitamin C). ROS generated by Ce6 was mainly derived from singlet oxygen via the Type 1 mechanism. The abundant ROS generation confirmed that Ce6-encapsulated nanoparticles are efficient for PDT application and accelerated hypoxia-boosted TPZ release.

According to our design, the hypoxic conditions created by PDT facilitate hydrophobic NI conversion to hydrophilic AI and boost micelle disassembly and cargo release. Therefore, we measured the variability in the diameter of NI-containing nanoparticles after 660-nm laser exposure. The diameters of NP_CT, ^SANP_CT, and ^DANP_CT significantly decreased to ∼45 nm following photosensitization (Figure 3A), and negligible changes were observed in the dark. We quantified the TPZ release profiles with or without PDT via fluorescence spectrometry. At 48 h, there were 75.96% ± 3.94%, 72.31% ± 2.14%, and 73.14% ± 2.96% TPZ leakages from NP_CT, ^SANP_CT, and ^DANP_CT after laser treatment, respectively (Figure 3B). In contrast, less than 12.50% of the total TPZ was detected without laser irradiation, and there was no significant difference in TPZ release rates. TPZ release from ^DANP_CT exhibited a power density-dependent pattern, and PDT resulted in 73.66% ± 3.34%, 49.53% ± 2.34%, and 30.21% ± 2.09% of TPZ liberation at different power densities (Figure 3C). The 660-nm laser on/off cycle induced controlled pulses of TPZ release from ^DANP_CT (Figure 3D). The hierarchy of pH_e and hypoxic conditions enabled TAT ligand presentation and cargo release, promoting the accumulation of active drug content at the target site.

FIGURE 3

FIGURE 3. (A) Diameter change in NP_CT, ^SANP_CT, and ^DANP_CT after exposure to 660-nm near infrared light. (B) Cumulative TPZ release profile of NP_CT, ^SANP_CT, and ^DANP_CT. The power density of 660-nm laser was 500 mW/cm². *p < 0.05. (C) Cumulative TPZ release profile of ^DANP_CT at 500 mW/cm², 200 mW/cm², and 100 mW/cm² or in the dark. *p < 0.05. (D) Pulsed 660-nm laser-triggered TPZ release from ^DANP_CT. The samples were exposed to laser at the predetermined time intervals indicated by the black arrows.

Cellular uptake of ^DANP_CT at pH 6.5

To track the TAT presentation of ^DANP_CT under acidic conditions to facilitate cellular internalization, MCF-7 cells were cultured and treated with NP_CT, ^SANP_CT, and ^DANP_CT for 4 h. The internalized NP content was analyzed by FACS, which revealed limited cellular uptake with ^SANP_CT pretreatment at pH 7.4 and 6.5, suggesting reduced interaction between masked TAT-induced and targeted cells (Figure 4A). Due to the pH_e-sensitive TAT, the intracellular ^DANP_CT content was significantly higher at pH 6.5 than at pH 7.4, comparable to that of NP_CT. Following cell lysis, we used HPLC to detect intracellular TPZ concentration and found that the internalized TPZ of ^DANP_CT increased from 0.69 ± 0.07 μg/mg protein (pH 7.4) to 1.39 ± 0.09 μg/mg protein (pH 6.5) (Figure 4B). However, there was no noticeable change in the NP_CT and ^SANP_CT groups at neutral or acidic pH. The pH-induced ^DANP_CT pattern was confirmed by confocal imaging. Compared to the weakened signals in the ^SANP_CT groups, significantly stronger fluorescence was observed when cells were incubated with ^DANP_CT pretreated at pH 6.5 (Figure 5). These results verified that the penetration capacity of masked TAT was specifically activated by the extracellular pH microenvironment.

FIGURE 4

FIGURE 4. (A) Intracellular fluorescence of NP_CT, ^SANP_CT, and ^DANP_CT in MCF-7 cells at pH 7.4 or 6.5. (B) Intracellular Ce6 concentration in MCF-7 cells at different pH conditions. *p < 0.05.

FIGURE 5

FIGURE 5. CLSM observation of NP_CT, ^SANP_CT, and ^DANP_CT on MCF-7 cells at either pH 7.4 or 6.5. Cell nuclei and F-actin were stained by DAPI (blue) and phalloidin-Alexa Fluor 488 (green), respectively. The scale bar is 20 μm.

Cell killing in vitro

The biocompatibility of non-loaded NP, ^SANP, and ^DANP was evaluated by CCK-8 assay, which showed no notable cytotoxicity in MCF-7 cells at the highest concentration of 500 μg/mL (Supplementary Figure S4). For chemo-PDT effectiveness, cells were incubated with NP_CT, ^SANP_CT, or ^DANP_CT, exposed to 660-nm light for 20 min, and then cultured at different O₂ concentrations. Without laser exposure, NP_CT, ^SANP_CT, and ^DANP_CT induced low toxicity even under hypoxic conditions because of the absence of the PDT effect and TPZ (HAP) release (Figures 6A,B). However, laser irradiation-triggered cell killing occurred in all groups at comparable levels regardless of pH or O₂ conditions. Hypoxic culture reduced cell viability, indicating that TPZ was reduced to cytotoxic radicals that interacted with the nuclear DNA. Compared to the viability of MCF-7 cells treated with ^DANP_CT at pH 7.4, acidic treatment promoted cell killing with 51.07% ± 6.98% cell viability (Ce6 4.0 μg/mL) under normoxic conditions. This difference is attributable to the reactivable TAT ligands and improved Ce6 and TPZ internalization. Under hypoxic conditions, the viabilities of NP_CT + L and ^DANP_CT + L groups at acidic pH were 21.90% ± 2.30% and 26.67% ± 4.29%, respectively, 0.50- and 0.61-fold lower than those of ^SANP_CT + L. Accordingly, the interactions between PDT and hypoxia-activated chemotherapy indicate that ^DANP_CT could serve as a robust delivery platform for precise cancer therapy.

FIGURE 6

FIGURE 6. Relative MCF-7 cell viabilities after incubation with NP_CT, ^SANP_CT, or ^DANP_CT at pH 7.4 (A) or 6.5 (B). *p < 0.05.

Pharmacokinetic and biodistribution of ^DATAT-NP_Ce6 in vivo

With pH_e-sensitive DA masking, the penetrating ability of the TAT ligand in ^DANP_CT was temporally blocked in the bloodstream, limiting phagocytosis. We measured the plasma concentrations of Ce6 following the intravenous injection of different formulations (Figure 7A). NP_CT with bare TAT ligands was rapidly cleared from the circulation, yielding a Ce6 concentration of 0.63 ± 0.45 μg/mL at 72 h post-injection. In contrast, both ^SANP_CT and ^DANP_CT substantially prolonged the Ce6 circulation, consistent with prior reports (Gao et al., 2017; Zhang et al., 2022). Compared to ^SANP_CT administration, the Ce6 plasma concentration in the ^DANP_CT group at 72 h post-injection was reduced from 2.71 ± 1.06 to 1.81 ± 0.54 μg/mL. The pharmacokinetic difference between ^SANP_CT and ^DANP_CT could be explained by the slight DA degradation at pH 7.4 (Supplementary Figure S4). We calculated the pharmacokinetic parameters of these nanocarriers using a non-compartmental model (Figures 7B,C) and found that the AUC_0-t values of ^SANP_CT and ^DANP_CT were 3.08- and 2.32-fold higher than those of NP_CT, respectively.

FIGURE 7

FIGURE 7. (A) Ce6 content in plasma vs. time, following i.v. injection of free Ce6, NP_CT, ^SANP_CT, or ^DANP_CT (n = 4). The area under the curve (B) and half-life (C) of free Ce6, NP_CT, ^SANP_CT, or ^DANP_CT calculated using a non-compartmental model. *p < 0.05. (D) Ce6 accumulation in MCF-7 tumor at 12, 24, and 48 h post-injection. *p < 0.05. (E) Ce6 distribution in major organs of MCF-7 tumor-bearing mice at 48 h post-injection.

Next, NP_CT, ^SANP_CT, or ^DANP_CT were i.v. injected into BALB/c nude mice bearing MCF-7 xenografts to evaluate their biodistribution, especially toward tumor tissues. After administration, the mice were euthanized at predetermined timepoints, and the Ce6 content in different organs was analyzed by HPLC. ^DANP_CT had the most preferential retention in tumor tissues at 48 h compared to NP_CT and ^SANP_CT due to the pH_e-triggered TAT-presenting effect (Figure 7D). Although ^SANP_CT showed more advanced tumor extravasation via EPR based on the best circulation pattern, stable SA modification impeded TAT ligand interaction and function in the tumor cells, resulting in insufficient tumor accumulation. The amounts of ^DANP_CT quantified by Ce6 content were 2.32% ± 0.29%, 3.11% ± 0.23%, and 2.47% ± 0.21% ID per gram of tumor at 12, 24, and 48 h, respectively. The nano-sized delivery systems NP_CT, ^SANP_CT, and ^DANP_CT accumulated in the liver and spleen, both components of the reticuloendothelial system (Figure 7E).

Therapeutic efficacy of ^DANP_CT in vivo

Encouraged by the excellent in vitro performance, we evaluated the in vivo antitumor efficacy of ^DANP_CT. MCF-7 tumor-bearing mice were randomly divided and treated via i.v. injection with (1) 0.9% NaCl, (2) free Ce6 + TPZ + PDT, (3) NP_CT + PDT, (4) ^SANP_CT + PDT, and (5) ^DANP_CT + PDT. The equivalent TPZ dose was 5.0 mg/kg, and the tumor size was recorded every 3 days. Tumor volume in the saline group rapidly increased to 1986.15 mm³ at the end of treatment (Figure 8A). Because of their prolonged blood circulation and improved biodistribution, NP_CT and ^SANP_CT significantly inhibited tumor growth after PDT compared to the free Ce6 + TPZ + PDT. Notably, the smallest tumor volumes in the ^DANP_CT + L group revealed that this treatment yielded the best therapeutic effect, with an average tumor volume of only 567.78 mm³ on day 24. The tumor weight after euthanizing confirmed these results (Figure 8B). Tumor mass in the ^DANP_CT + PDT group was 0.70- and 0.52-fold lower than that in the NP_CT + L and ^SANP_CT + L groups, respectively. In addition, the body weight curves in Supplementary Figure S5 show that the ^DANP_CT + L group did not experience a decline in the body weight, suggesting the biosafety of ^DANP_CT in vivo. H&E staining (Figure 8C), routine blood count (Supplementary Table S1), and ELISA tests (Supplementary Figure S6) for liver/kidney damage after treatment showed no significant lesions or inflammation in any groups, validating the biocompatibility of the ^DANP_CT system.

FIGURE 8

FIGURE 8. (A) Tumor growth curve of the MCF-7 tumor-bearing BALB/c nude mice treated with various formulations. The mice bearing intravenous injections were performed on days 0, 7, 14, and 21. *p < 0.05. (B) MCF-7 tumor mass after the treatment. *p < 0.05. (C) Tumor images at the end of the treatment. (D) H&E staining of tumors and major organs at the end of the tumor treatment.

Conclusion

In this work, a hierarchically responsive nanocarrier ^DANP_CT was fabricated to spatially control TAT presentation in tumor sites for PDT-initiated, hypoxia-activated cancer therapy. ^DANP_CT exhibited advanced stability at neutral pH and rapidly reactivated TAT function in response to pH_e, specifically accelerating internalization by tumor cells. Upon 660-nm laser irradiation, Ce6-based PDT produced cell-killing ROS and consumed surrounding O₂ to generate hypoxic conditions that stimulated ^DANP_CT disassembly and TPZ liberation. Chemotherapy with TPZ was enhanced by the aggravated hypoxia in tumor tissues. The biosafety studies of ^DANP_CT showed excellent in vivo biocompatibility with healthy organs. On the other hand, further studies on the feeding ratio of TAT-PEG-b-PHEP, PEG-b-P (AEP-g-NI), Ce6, and TPZ during the preparation of ^DANP_CT is necessary for optimal therapeutical efficacy in vivo. This work contributes to the rational design of tumor microenvironment-responsive nanocarriers for precise and cascade cancer therapies.

Data availability statement

The original contributions presented in the study are included in the article/Supplementary Material; further inquiries can be directed to the corresponding authors.

Ethics statement

The animal study was reviewed and approved by the Institutional Animal Care and Use Committee at Tianjin Medical University General Hospital.

Author contributions

Conceptualization, ZZ, AG, and CS; methodology, ZZ and JF; validation, ZZ, JF, and TZ; formal analysis, TZ and AG; investigation, ZZ and JF; data curation, AG; writing—original draft preparation, ZZ, JF, and AG; writing—review and editing, AG and CS; supervision, CS; funding acquisition, ZZ and CS. All authors contributed to the article and approved the submitted version.

Funding

This work was supported by the National Natural Science Foundation of China (82071907 and 82271937), Natural Science Foundation of Tianjin (18JCYBJC25100), Health science and Technology Project of Tianjin (MS20022), Tianjin Key Medical Discipline (Specialty) Construction Project (TJYXZDXK-001A), and Wu Jieping Medical Foundation-Special Fund for Clinical Research (320.6750.2022-3-5).

Conflict of interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Publisher’s note

All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors, and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.

Supplementary material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fbioe.2023.1197404/full#supplementary-material

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