Redox-sensitive Polymeric Micelles With Aggregation-induced Emission for Bioimaging and Delivery of Anticancer Drugs

doi:10.21203/rs.3.rs-68528/v1

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Redox-sensitive Polymeric Micelles With Aggregation-induced Emission for Bioimaging and Delivery of Anticancer Drugs

https://doi.org/10.21203/rs.3.rs-68528/v1

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published 07 Jan, 2021

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Background: Nano-drug delivery systems show considerable promise for effective cancer therapy. Polymeric micelles have attracted extensive attention as practical nanocarriers for target drug delivery and controlled drug delivery system, however, the distribution of micelles and the release of the drug are difficult to trace in cancer cells. Therefore, the construction of a redox-sensitive multifunctional drug delivery system for intelligent release of anticancer drugs and simultaneous diagnostic imaging and therapy remains an attractive research subject.

Results: To construct a smart drug delivery system for simultaneous imaging and cancer chemotherapy, mPEG-ss-Tripp was prepared and self-assembled into redox-sensitive polymeric micelles with a diameter of 105 nm that were easily detected within cells using confocal laser scanning microscopy based on aggregation-induced emission. Doxorubicin-loaded micelles rapidly released the drug intracellularly when GSH reduced the disulfide bond. The drug-loaded micelles inhibited tumor xenografts in mice, while this efficacy was lower without the GSH-responsive disulfide bridge. These results establish an innovative multi-functional polymeric micelle for intracellular imaging and redox-triggered drug deliver to cancer cells.

Conclusions: A novel redox-sensitive drug delivery system with AIE property was constructed for simultaneous cellular imaging and intelligent drug delivery and release. This smart drug delivery system opens up new possibilities for multifunctional drug delivery systems.

Nanoscience

Polymeric micelles

Redox-sensitive

Aggregation-induced emission

Drug delivery

Bioimaging

Nanocarriers have attracted extensive attention as practical methods for target drug delivery and controlled drug delivery system for highly efficient anticancer therapy.^1,2 Among these carriers, polymeric micelles, self-assembling from amphiphilic block copolymers, are of great interest and importance, because of several merits such as the enhanced water solubility, improved biocompatibility, decreased side effects, passive accumulation of the drugs in the tumor tissues and prolonged circulating time. Although considerable efforts on developing efficient polymeric micelles have been made in recent years, especially, several polymeric micelles have been reached to clinical trials,^3,4 the distribution of micelles and the release of the drug is difficult to trace in cancer cells.^5,6 Therefore, the development of theranostic nanoparticles with integrated with diagnostic imaging and therapeutic capability is urgent needed for drug delivery systems.^7-9 However, the classical methodology that encapsulates traditional fluorescent dyes into the core of nanoparticles,^10-12 often suffered from fluorescence quenching of fluorescence agents in an aggregated state because of the aggregation caused quenching (ACQ) effect, which greatly reduces the fluorescence intensity and impedes the imaging effect, limiting their biomedical applications.^13-15 In 2001, Tang developed a class of novel category of fluorophores with aggregation-induced emission (AIE) characteristics, which exhibit high emission efficiencies in an aggregated state.^16,17 Recently, the relevant AIE probes have been employed for cell imaging.^18-21 This unique property makes the AIE-active polymeric micelles as the drug nanocarriers available for simultaneous cancer diagnostic and therapy.

When the drug-loaded micelles reaches the target tumor tissues, rapid release of the drug is required to improve antitumor efficacy and circumvent drug resistance in pathological cells. In this regard, smart polymeric micelles with stimuli-sensitive features have been explored for target site-triggered drugs release in response to appropriate environment of tumor tissues.^22-26 Among various stimuli-sensitive antitumor drug nanocarriers, redox-sensitive disulfide linkage contained polymeric micelles have attracted more and more attention for controlled delivery and intelligent release of anticancer drugs. Disulfide linkage of the polymeric micelles can be quickly cleaved by reductive substance glutathione (GSH) via thiol-disulfide exchange²⁷ at high concentration of GSH in the intracellular environment of tumor cells (approximately 2-10 mM), while relatively stable at a low concentration of GSH in the extracellular environment (approximately 2-20 µM).^24,28 Moreover, the GSH concentration in tumor cells is typically at least four times higher than the values of healthy cells.^29,30 In this context, the construction of a redox-sensitive multifunctional drug delivery system taking advantage of this characteristic for intelligent release of anticancer drugs and simultaneous cancer diagnostic and therapy remains an attractive research subject.

In this study, a redox-sensitive drug delivery system with AIE property was constructed for simultaneous cellular imaging and intelligent drug delivery and release. We conjugated the AIE fluorophore Tripp to methoxy-PEG via a redox-sensitive disulfide bond. As a control, we also prepared redox-insensitive mPEG-Tripp. We anticipated that the synthetic polymer molecule would self-assemble into micelles in which mPEG would serve as a biocompatible shell that would circulate in the blood for a long time, and the hydrophobic AIE core would allow cellular imaging and loading of hydrophobic anticancer drug such as doxorubicin (DOX). The disulfide bridge, in turn, would help ensure rapid release of the drug within tumor cells but not in the circulation (Scheme 1).

Materials

Methoxypoly (ethylene glycol) (mPEG; Mw 2000 g/mol), succinic anhydride (SAA), chloroform-D (CDCl₃, 99.8%) and deuterated dimethyl sulphoxide (DMSO-d₆) were purchased from Sigma-Aldrich (Shanghai, China); 1-ethyl-(3-dimethylaminopropyl)-carbodiimide hydrochloride (EDC·HCl), methyl 4-aminobenzoate and 1-hydroxy-benzotriazole monohydrate (HOBt), from GL Biochem (Shanghai, China); tetramethylethylenediamine, N,N-diisopropyl ethylamine (DIEA) and 4-dimethylaminopyridine (DMAP), from Aladdin Chemistry (Shanghai, China); 1,3-dicyclohexylcarbodiimide (DCC) and cystamine dihydrochloride, from Asta Tech Biopharm (Chengdu, China); and doxorubicin hydrochloride (DOX·HCl), from Shanghai Yingxuan Chempharm (Shanghai, China). DOX was deprotonated as reported.³¹ All solvents were obtained from Chengdu Kelong Chemical (Chengdu, China) and purified before use. Dulbecco's Modified Eagle's Medium (DMEM), Roswell Park Memorial Institute (RPMI) 1640 medium, fetal bovine serum (FBS), and the cell counting kit-8 (CCK-8) were purchased from Life Technologies (Gibco, USA).

Synthesis of redox-sensitve amphiphiles mPEG-ss-Tripp

Synthesis of mPEG-SAA

The mPEG (0.2 g, 0.1 mmol) and SAA (0.05 g, 0.5 mmol) were dissolved in 60 mL of anhydrous CH₂Cl₂ with strong stirring. Pyridine (0.4 mL) was added dropwise to the mixture on an ice bath. The mixture was stirred at room temperature for 48 h. An appropriate amount of acetic acid was added to the reaction system under stirring in order to neutralize salts produced in the system. The precipitate was removed by filtration, the filtrate was evaporated and the crude product was precipitated in a large volume of cold diethyl ether. This purification procedure was repeated several times to yield mPEG-SAA.

Synthesis of mPEG-ss-NH₂

The mPEG-SAA (0.81 g, 0.4 mmol), EDC·HCl (0.32 g, 1.6 mmol) and HOBT (0.22 g, 1.6 mmol) were dissolved in 60 mL of DMF and stirred at room temperature for 3 h. To the solution was added

cystamine dihydrochloride (0.14 g, 0.6 mmol), and the mixture was vigorously stirred at room temperature for 48 h. Then the mixture was filtered and concentrated under reduced pressure. The dark brown residual oil was redissolved in CH₂Cl₂, and the organic phase was extracted three times with a saturated aqueous solution of sodium chloride, dried with anhydrous MgSO₄ overnight and concentrated. The crude product was precipitated three times in cold anhydrous diethyl ether and dried under vacuum to obtain light-yellow solid mPEG-ss-NH₂.

Synthesis of mPEG-ss-Tripp

The mPEG-ss-NH₂ (0.45 g, 0.2 mmol), Tripp-COOH³² (0.21 g, 0.6 mmol), EDC·HCl (0.16 g, 0.8 mmol) and HOBT (0.11 g, 0.8 mmol) were added to 60 mL of DMF, then DIEA (0.2 mL, 1.2 mmol) was injected into the solution, and the mixture was stirred at room temperature for 48 h. The solvent was evaporated under reduced pressure, and the residue was dissolved in CH₂Cl₂. The organic phase was washed three times with a saturated aqueous solution of sodium chloride and dried over anhydrous MgSO₄. The filtrate was concentrated and precipitated twice in cold diethyl ether to yield mPEG-ss-Tripp.

Characterization

Products were analyzed in DMSO-d₆using ¹H NMR (Ascend 400 MHz, Bruker), with tetramethylsilane as an internal reference. Micelle size and size distribution were analyzed by dynamic light scattering (Malvern ZetasizerNano ZS, UK). Micelle morphology was observed using scanning electron microscopy (S4800, Hitachi, Japan). Samples were prepared for electron microscopy by dipping a silicon pellet into a solution of freshly prepared micelles, then drying the pellet overnight at room temperature.

Preparation of drug-loaded micelles

Drug-loaded micelles DOX/mPEG-ss-Tripp were prepared using a dialysis method. Briefly, freeze-dried amphiphilic mPEG-ss-Tripp (10 mg) and DOX (2.5 mg) were co-dissolved in 1 mL of DMSO, dispersed slowly into 10 mL of deionized water and stirred vigorously overnight. Then, the mixtures were dialyzed against deionized water at 4 °C for 12 h in dialysis tubing (Spectra/Por) with a molecular weight cut-off of 1 kDa. The solution was removed from the

dialysis tubing, centrifuged and freeze-dried. Redox-insensitive DOX/mPEG-Tripp micelles were prepared in the same way.

DOX content of drug-loaded micelles was determined by UV/vis spectroscopy (Specord 200 PLUS, Germany) at 480 nm using a standard calibration curve obtained from solutions containing different concentrations of DOX in DMSO. Solutions were shielded from light. Drug loading content (DLC) and encapsulation efficiency (DLE) were calculated according to the following formulas:

DLC (%) = (weight of loaded DOX/weight of drug-loaded micelle) × 100%

DLE (%) = (weight of loaded DOX /weight of drug in feeding) × 100%

In vitro drug release

Profiles of DOX release from micelles were investigated in phosphate-buffered saline (PBS; pH 7.4, ionic strength = 0.01 M) alone or supplemented with 2 μM, 2 mM or 10 mM GSH. Briefly, 1 mL of

drug-loaded micelles were transferred into dialysis tubes (Spectra/Por) with a molecular weight cut-off of 1 kDa and immersed in 25 mL of release medium in vials with continuous shaking at 120 rpm and 37 °C. At predetermined intervals, 1 mL of release medium was taken out and replaced with an equal volume of fresh medium. The released DOX was detected using a fluorescence spectrometer (F-7000, Hitachi, Japan) with excitation at 480 nm and emission at 550 nm. The release experiments were conducted in triplicate under sink conditions, and average values with standard deviations were presented.

In vitro cytotoxicity and antitumor efficacy

Medium was removed and replaced with 100 µL of medium containing different concentrations of blank micelles. Then the cells were incubated for another 48 h, the medium was removed, the wells were rinsed three times with PBS, and CCK-8 solution (100 µL, volume fraction, 10%) was added to each well. The cells were incubated another 2 h in the dark, and absorbance was measured at 450 nm using a microplate reader (Thermo Scientific MK3, USA).

Antitumor activity of drug-loaded micelles against 4T1 cells was also evaluated using the CCK-8 assay. Cells were seeded and incubated for 24 h in 96-well plates as described above, then free DOX·HCl or DOX-loaded micelles in culture medium were added at various DOX concentrations (0.001-100 μg/mL) and the cells were incubated another 48 h. After that, the cells were subjected to the CCK-8 assay as described above.

In vitro drug release

Profiles of DOX release from micelles were investigated in phosphate-buffered saline (PBS; pH 7.4, ionic strength = 0.01 M) alone or supplemented with 2 μM, 2 mM or 10 mM GSH. Briefly, 1 mL of drug-loaded micelles were transferred into dialysis tubes (Spectra/Por) with a molecular weight cut-off of 1 kDa and immersed in 25 mL of release medium in vials with continuous shaking at 120 rpm and 37 °C. At predetermined intervals, 1 mL of release

medium was taken out and replaced with an equal volume of fresh medium. The released DOX was detected using a fluorescence spectrometer (F-7000, Hitachi, Japan) with excitation at 480 nm and emission at 550 nm. The release experiments were conducted in triplicate under sink conditions, and average values with standard deviations were presented.

In vitro cytotoxicity and antitumor efficacy

The biocompatibility of blank micelles was evaluated using the CCK-8 assay. 293T human embryonic kidney cells and 4T1 breast cancer cells were separately seeded in 96-well plates (6×10³ cells per well) in 100 μL of culture medium and incubated for 24 h. Medium was removed and replaced with 100 µL of medium containing different concentrations of blank micelles. Then the cells were incubated for another 48 h, the medium was removed, the wells were rinsed three times with PBS, and CCK-8 solution (100 µL, volume fraction, 10%) was added to each well. The cells were incubated another 2 h in the dark, and absorbance was measured at 450 nm using a microplate reader (Thermo Scientific MK3, USA).

DOX-loaded micelles in culture medium were added at various DOX concentrations (0.001-100 μg/mL) and the cells were incubated another 48 h. After that, the cells were subjected to the CCK-8 assay as described above.

Cellular uptake of micelles

Uptake of micelles by 4T1 cells was analyzed using confocal laser scanning microscopy and flow cytometry. Cells in logarithmic growth were seeded in 35-mm confocal dishes (2×10⁴ mL^-1 cells per well) and incubated for 24 h. Then the medium was replaced with blank or DOX-loaded micelles (10 μg/mL DOX) in culture medium and cells were incubated for 1 or 3 h. The medium was removed and cells were washed three times with cold PBS, then examined using confocal laser scanning microscopy with excitation at 480 nm and emission at 590 nm.

For the flow cytometry tests, 4T1 cells were seeded in 6-well plates (1×10⁵ mL^-1 cells per well), incubated for 24 h, then treated for 1 or 3 h with free DOX·HCl or DOX-loaded micelles (10 μg/mL DOX). After that, medium was removed and cells were washed three times in PBS and harvested by trypsin treatment. Finally, cells were centrifuged (1000 rpm, 5 min), resuspended in PBS, and analyzed using flow cytometry ( BD FACSCanto II, USA ).

In vivo toxicity and antitumor efficacy

All animal experiments were performed according to institutional guidelines and the recommendations of the US National Institutes of Health for the care and use of research animals. Male BALB/c mice (18-20 g) were purchased from West China Experimental Animal Culture Center of Sichuan University (Chengdu, China). 4T1 cells (1×10⁶) were injected subcutaneously into the right flank, and when the inoculated tumors reached a volume of 100-200 mm³, the animals were randomized to receive one of the following treatments (n = 8 per group): saline, DOX·HCl, DOX/mPEG-ss-Tripp micelles, or DOX/mPEG-Tripp micelles (DOX always at 5 mg/kg body). Treatments were delivered intravenously via the tail vein every 3 days for 4 treatments. Tumor volume and body weight were monitored at prescribed time intervals, and tumor volume was calculated using the formula: V (mm³) = 1/2 × ab²,

where a and b are the largest and smallest diameters of the tumor, respectively.

At 21 d after the fourth treatment, all mice were sacrificed. Organs including heart, liver, spleen, lung, kidney and tumor were excised from each mouse and fixed in 4% formaldehyde. Representative tissues were paraffin-embedded, sectioned, stained with hematoxylin and eosin and examined under a light microscope. Blood was assayed using standard serum tests performed by Chengdu Lilai Biotechnology (Chengdu, China) Tumor sections were immunostained with monoclonal antibody against Ki-67 to assess tumor proliferation, while sections were assayed by terminal deoxynucleotidyl transferase-mediated deoxyuridine triphosphate nick-end labeling (TUNEL) to assess the level of apoptosis.

Statistical analysis

All data are presented as mean ± standard deviation (SD). Inter-group differences were assessed for significance using Student’s t test, and p < 0.05 was defined as significant.

Characterization of mPEG-ss-Tripp and mPEG-Tripp

The conjugates mPEG-ss-Tripp and mPEG-Tripp were synthesized conveniently (Scheme 2), and the chemical structures of intermediates and final copolymers were confirmed by ¹H NMR. The protons of mPEG-SAA showed chemical shifts at  = 3.35-3.40 ppm (1), =3.50-3.80 ppm (2, 3) and = 2.55-2.67 ppm (4, 5) (Figure 1A). Conjugation with cystamine via an amido linkage gave peaks at =2.60-3.00 ppm (7, 8), which were assigned to the protons of -CH₂CH₂ in cystamine (Figure 1B). The appearance of peaks at =7.70-7.80 ppm, attributed to an amide bond, confirmed that the cystamine segment was introduced into mPEG-SAA. The appearance of peaks at δ = 6.50 ppm (14) and δ = 7.20-7.89 ppm (9-13), attributed to the pyrrole and benzene rings, respectively (Figure 1C), confirmed the synthesis of the amphiphilic polymer mPEG-ss-Tripp. In mPEG-Tripp, peaks at δ = 3.35 ppm (1) and δ = 3.6 ppm (2) were assigned, respectively, to protons in the terminal CH₃ and OCH₂CH₂ in PEG. The other two peaks at δ = 6.50 ppm (6) and δ = 7.08-7.73 ppm (3, 4, 5, 7, 8) were attributed, respectively, to the pyrrole and benzene rings (Figure S1).

Preparation of blank and DOX-loaded micelles

Based on dynamic light scattering, hydrodynamic diameters of blank micelles were 102 nm for mPEG-ss-Tripp and 99 nm for mPEG-Tripp (Figure 2A), and loading the two micelles with DOX increased their respective diameters to 122 and 117 nm (Figure 2B). With or without drug, micelles showed narrow size distributions, with a polydispersity index of 0.17-0.21. Scanning electron microscopy showed uniform, spherical sizes that were consistent with the results of dynamic light scattering. These sizes can help nanoparticles to evade scavenging by mononuclear phagocytes as well as to target tumors passively through enhanced permeability and retention.^33-35

Micelles of mPEG-ss-Tripp and mPEG-Tripp showed respective DLCs of 10.5% and 10.1%, and respective DLEs of 71.6% and 69.5%. The relatively high DLC of micelles is due to the introduction of π-conjugated moieties (Tripp), which enhances π-π stacking between DOX and amphiphilic polymers. After excitation at 485 nm, free DOX·HCl emitted intense fluorescence from 500 to 700 nm, while DOX/mPEG-ss-Tripp and DOX/mPEG-Tripp at the same DOX concentration (25 μg/mL) emitted much weaker signal (Figure S2). This quenching is presumably due to the π-π stacked DOX.³⁶

AIE behavior of mPEG-ss-Tripp

Since the Tripp-COOH groups, as the hydrophobic moieties in the amphiphile mPEG-ss-Tripp, are trapped inside the micellar cores during micelle formation, the aggregation state of Tripp-COOH molecules should trigger AIE. We confirmed this in vitro using a fluorescence assay. The mPEG-ss-Tripp dissolved in DMSO showed weak fluorescence, which increased dramatically when water was added to the DMSO solution (Figure 3A). When the water fraction reached 99% (v/v), fluorescence intensity of mPEG-ss-Tripp was nearly 74-fold stronger than in 100% DMSO (Figure 3B). These results confirm the AIE of mPEG-ss-Tripp micelles.

In vitro drug release

In vitro DOX release from micelles was investigated in the presence of GSH at extracellular levels (2 μM) and intracellular levels (2-10 mM). Release from mPEG-ss-Tripp micelles increased with increasing GSH concentration (Figure 3C), suggesting that GSH

triggered release. For example, after 72 h, only 40.5% of DOX was released from mPEG-ss-Tripp micelles in the presence of 2 μM GSH, compared to 37.6% of DOX in the absence of GSH. In contrast, after only 24 h, 81.4% was released in the presence of 10 mM GSH and 75.2% in the presence of 2 mM GSH, and these percentages increased to 96.2% and 93.0% at 72 h. These results suggest that, as desired, our nanosystem delivers drug cargo selectively within cells, in response to the much higher intracellular GSH concentration. The disulfide linkage is essential for this redox-sensitive, even after 72 h, only 35.9% of DOX was released from mPEG-Tripp micelles in the presence of 10 mM GSH.

Change in micelle size in response to GSH

Dynamic light scattering showed that mPEG-ss-Tripp micelles swelled rapidly in the presence of GSH: in the presence of 0.5 mM GSH, average size increased from 105 to 342 nm within 5 h; in the presence of 10 mM GSH, average size increased from 342 to 531 nm in 5 h, and to >1600 nm in 12 h (Figure 4A). In contrast, the size of mPEG-Tripp micelles changed little even after 12 h in the presence of 10 mM GSH. Consistent with GSH-triggered micelle opening and drug release, the count rate of the mPEG-ss-Tripp micelles decreased with time and with increasing GSH concentration (Figure 4B). These results suggest that 10 mM GSH can trigger complete dissolution of mPEG-ss-Tripp micelles.

In vitro cytotoxicity of micelles

Blank micelle concentrations up to 1 mg/mL showed negligible toxicity against 293T and 4T1 cells after 48 h incubation, based on the CCK-8 assay (Figure 5A and 5B). At the same time, DOX-loaded micelles reduced the viability of 4T1 cells, although their half-maximal inhibitory concentrations (IC₅₀) were higher than for free DOX (mPEG-ss-Tripp, 1.65 μg/mL; mPEG-Tripp, 12.74 μg/mL; free DOX·HCl, 0.71 μg/mL (Figure 5C and 5D). The greater anticancer activity of free DOX likely reflects its ability to enter cells by passive diffusion. The much greater anticancer activity of mPEG-ss-Tripp than mPEG-Tripp likely reflects that cleavage of the disulfide bond within cells triggers faster drug release from the micelle interior than simple diffusion.

Intracellular imaging of AIE micelles in vitro

Uptake of micelles and intracellular release of drug were analyzed using confocal fluorescence microscopy and flow cytometry on the basis of AIE signal. Within 1 h of incubation with blank or DOX-loaded micelles, blue AIE fluorescence was clearly visible within the cytoplasm of 4T1 cells (Figure 6A), suggesting rapid internalization of micelles via endocytosis. Cells incubated with free DOX·HCl showed red fluorescence mainly in nuclei, reflecting the excellent aqueous solubility of DOX and its ability to enter cells and nuclei by passive diffusion. However, for the DOX-loaded micelles, most red fluorescence of DOX was concentrated in cytoplasm;

only weak red fluorescence was observed in nuclei. Both red and blue fluorescence intensity were higher at 3 h than at 1 h, confirming that more drug-loaded micelles were internalized into cells and sustainably released the drug intracellularly. These experiments confirm that DOX-loaded micelles can be used for bioimaging and drug delivery.

The results of confocal microscopy were confirmed using flow cytometry. While control cells showed only autofluorescence, cells treated with DOX·HCl showed the strongest fluorescence, followed by cells treated with mPEG-ss-Tripp and finally cells treated with mPEG-Tripp (Figure 7A and 7B).

In vivo toxicity and antitumor efficacy of micelles

Tumor-bearing BALB/c mice were treated every 3 days with saline, DOX·HCl or DOX-loaded micelles. By 21 days of treatment, the tumor volume in the saline group had increased rapidly (Figure 8A), indicating that the saline did not have any therapeutic effect. DOX·HCl and DOX-loaded micelles, in contrast, strongly inhibited tumor growth. Notably, treatment with mPEG-ss-Tripp group showed better anticancer activity than mPEG -Tripp group. Over the same period, animals treated with free DOX lost considerable body weight (Figure 8B), indicating serious systemic toxicity, whereas animals treated with DOX-loaded micelles did not. These results suggest that loading DOX into micelles can substantially reduce its toxicity. Consistent with this idea, all mice treated with DOX-loaded micelles survived for the entire period of 33 days, whereas 40% of mice treated with free DOX·HCl died within 18 days (Figure 8C).

Serum biochemistry assays confirmed that free DOX·HCl was strongly toxic, which was reflected in elevated aspartate transaminase (AST), alanine aminotransferase (ALT) and alkaline phosphatase (ALP) (Figure 8D). Indices in animals treated with DOX-loaded micelles were close to those in the saline group, indicating that the DOX-loaded micelles did not obviously harm tumor-bearing mice.

Hematoxylin-eosin staining of tumor tissue showed nearly no apoptosis or necrosis in the saline group, while it showed tumor necrosis with hemorrhage in the groups treated with free DOX·HCl or DOX-loaded micelles (Figure 9). Staining of slices from heart, liver, spleen, lung and kidney showed numerous pathological signs in animals treated with free DOX·HCl: dissolution of myocardial cytoplasma; swelling, shrinkage or disappearance of kidney glomerular cells; white pulp atrophy and splenic corpuscle disappearance in spleen; and lobular pneumonia in lungs. No obvious pathology was observed in any tissues examined from animals treated with DOX-loaded micelles.

Immunohistochemistry and TUNEL staining

Tissue sections stained against Ki-67 antigen as an index of tumor proliferation showed that mPEG-ss-Tripp micelles suppressed proliferation more than other treatments (Figure 10). These results confirm that the redox-sensitive of the drug delivery system can improve therapeutic efficacy in vivo.

These in vivo experiments indicate that mPEG-ss-Tripp micelles lead to substantially lower toxicity than free DOX·HCl and greater efficacy than redox-insensitive mPEG-Tripp micelles.

We have designed a novel redox-sensitive amphiphilic polymer with AIE character to realize a drug delivery system for simultaneous cellular imaging and cancer therapy. When loaded with DOX, the amphiphilic polymer can self-assemble into drug-loaded micelles, which release their therapeutic cargo rapidly in response to reduction of the disulfide linkage at the high GSH concentrations inside cells. The micelles can be tracked within cells by virtue of their AIE. Removing the redox-sensitive disulfide bridge makes drug delivery slower and less effective against tumors. These results open up new possibilities for multifunctional drug delivery systems.

Acknowledgements

Not applicable.

Authors′ contributions

All authors contributed signifcantly to this work. BH, ZZ, and NH conceived and designed the experiments. CS and JL performed the experiments. CS, JL, JW, PH, CL, LQ, LY analyzed the data. NH, BH and ZZ oversaw the design of the experiments, data analysis, and edited the manuscript. All authors read and approved the fnal manuscript.

Funding

The authors thank for the support of the collaborative fund of Luzhou Government and Southwest Medcial University (2019LZXNYDJ16), the Transformation Project of Science and Technology Achievements of Southwest Medical University (2018002) and the research fund of Southwest Medical University (2017-ZRQN-037).

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its additional file.

Ethics approval and consent to participate

All of the animal experiments were carried out in accordance with the guidelines issued by Southwest Medical University and were approved by the Ethical Committee of Southwest Medical University.

Content for publication

All authors agreed to submit this manuscript.

Competing interests

The authors declare that they have no competing interests.

Author details

¹Department of Pharmaceutical Sciences, School of Pharmacy, Southwest Medical University, Luzhou 646000, China. ²Affiliated Traditional Chinese Medicine Hospital, Southwest Medical University, Luzhou 646000, People’s China. ³Biological group, Beijing Huimin School, Beijing 100032, China. ⁴National Engineering Research Center for Biomaterials, Sichuan University, Chengdu 610064, China.

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