Multifunctional nanocomposites DDMplusAF inhibit the proliferation and enhance the radiotherapy of breast cancer cells via modulating tumor-promoting factors and metabolic reprogramming
Multifunctional nanocomposites DDMplusAF inhibit the proliferation and enhance the radiotherapy of breast cancer cells via modulating tumor-promoting factors and metabolic reprogramming
Tumor-promoting factors (TPF) and metabolic reprogramming are hallmarks of cancer cell growth. This study is designed to combine the newly synthesized two nanocomposites DDM (HA-FA-2DG@DCA@MgO) and AF (HA-FA-Amygdaline@Fe2O3) with fractionated doses of radiotherapy (6 Gy-FDR; fractionated dose radiotherapy) to improve the efficiency of chemo-radiotherapy against breast cancer cell lines (BCCs; MCF-7 and MDA-MB-231). The physicochemical properties of each nanocomposite were confirmed using energy dispersive XRD, FTIR, HR-TEM, and SEM. The stability of DDMPlusAF was also examined, as well as its release and selective cellular uptake in response to acidic pH. A multiple-MTT assay was performed to evaluate the radiosensitivity of BCCs to DDMPlusAF at 3 Gy (single dose radiotherapy; SDR) and 6 Gy-FDR after 24, 48, and 72 h. Finally, the anti-cancer activity of DDMPlusAF with 6 Gy-FDR was investigated via assessing the cell cycle distribution and cell apoptosis by flow cytometry, the biochemical mediators (HIF-1α, TNF-α, IL-10, P53, PPAR-α, and PRMT-1), along with glycolytic pathway (glucose, HK, PDH, lactate, and ATP) as well as the signaling effectors (protein expression of AKT, AMPK, SIRT-1, TGF-β, PGC-1α, and gene expression of ERR-α) were determined in this study.
Results
The stability of DDMPlusAF was verified over 6 days without nanoparticle aggregation. DDMPlusAF release and selectivity data revealed that their release was amenable to the acidic pH of the cancer environment, and their selectivity was enhanced towards BCCs owing to CD44 and FR-α receptors-mediated uptake. After 24 h, DDMPlusAF boosted the BCC radiosensitivity to 6 Gy-FDR. Cell cycle arrest (G2/M and pre-G1), apoptosis induction, modulation of TPF mediators and signaling effectors, and suppression of aerobic glycolysis, all confirmed DDMPlusAF + 6 Gy’s anti-cancer activity.
Conclusions
It could be concluded that DDMPlusAF exerted a selective cancer radiosensitizing efficacy with targeted properties for TPF and metabolic reprogramming in BCCs therapy.
Breast cancer (BC) is the most common malignancy in women and one of the three most common cancers worldwide, along with lung and colon cancer (Harbeck and Gnant 2017). Adenosine triphosphate (ATP; energy source for survival) is produced in normal cells via two pathways: glycolysis and mitochondrial oxidative phosphorylation (OXPHOS). However, even in an aerobic environment, cancer cells gain ATP from glycolysis rather than OXPHOS, despite the glycolysis producing 2 ATP less than the OXPHOS that generates 36 ATP per glucose molecule. Notably, mitochondrial OXPHOS is not necessarily defective in cancer cells, but cancer cells mostly depend on glycolysis due to its acceleration than OXPHOS in ATP generation, and this is favorable for growth and proliferation. This metabolic reprogramming is recognized as the Warburg effect, and it is the cancer hallmark that is induced by oncogenic events and aggressively contributes to cancer progression in a harsh microenvironment (Dias et al. 2019; Shiratori et al. 2019).
The tumor microenvironment (TME) is an immunosuppressive microenvironment generated by cancer cells to regulate tumor growth, promote tumor immune evasion, and serve as a source of tumor-promoting factors (TPF) (Whiteside 2008; Shi et al. 2020). TPF has included growth factors, cytokines, extracellular matrix proteins, and hypoxia challenge as well as p53, which promote growth, survival, and metastatic spread of cancer cells (Han et al. 2014; Owusu et al. 2017). The TME is the network of cells such as immune cells, cancer-associated fibroblasts, and promoting factors (i.e., cytokines, growth factors, and hormones) associated with the extracellular matrix and surrounding vasculature that encloses cancer cells. The formation of this TME essentially relies on tumor metabolism, and therefore, it is characterized by high acidity and hypoxia (Shi et al. 2020). Additionally, the study by Vaughan et al. (2013) demonstrated that aerobic glycolysis is induced by the expression of oncogene and TME mediators. Furthermore, aerobic glycolysis leads to the accumulation of lactate in the TME, which results in stabilization of hypoxia-inducible factor (HIF), and subsequently stimulates transforming growth factor- beta (TGF-β) that in turn enhances aerobic glycolysis (Hua et al. 2020). Moreover, among the numerous regulators or mediators of cancer metabolism, peroxisome proliferator-activated receptor-gamma coactivator-1 alpha (PGC-1α) is emerging as a promoter of carcinogenesis and an essential controller of multiple metabolic pathways in cancer (Tan et al. Full size image
The composition of the synthesized DDM sample is analyzed by EDX (Fig. 1b), where the presence of O, C, Cl, and Mg was confirmed, and the presence of Mg and O atoms was correlated to the core MgO-NPs. Moreover, the presence of O, C, and Cl corresponds to the DA, 2DG, HA, and FA multi-shell structures in the synthesized sample.
Elemental map**s were performed selectively on the synthesized DDM samples to further illustrate the core–shell structural features of the samples, and the images are depicted in Fig. 1c. These images demonstrated the existence of the elements Mg, C, Cl, and O, which agreed with the preceding EDX results. Furthermore, those elements were distributed uniformly. The images confirmed that both Mg (blue color) and O (green color) atoms were located in the same places, confirming the core structure, and the other layers (C, O, and Cl) indicate the distribution of the organic shells structure on the core MgO-NPs.
The SEM image of the synthesized DDM sample is shown in Fig. 1d. The surface behavior reveals dark layers that represent the outer shells (HA and FA; organic shells) with remarkable smooth agglomerates. This could be due to the occupation of a large number of layers at the grain boundary, which could control the grain growth. In addition, the MgO-NPs in the core represented the bright aggregate particles, confirming the promising core–shell structure.
An HR-TEM image of the core–shell structure of the synthesized DDM is shown in Fig. 1e. The synthesized composite possessed a semi-spherical structure with diameter sizes ranging from 149.36 to 97.43 nm, with an average size of 123.38 nm. It must be noted that the condensed particles were attributed to the core MgO-NPs while the faint layers corresponded to the shell layers of DDM, which were entirely validated by color in the map**/SEM images and indicated the successful formation of core–shell construction.
The FTIR spectrum of the synthesized DDM is presented in Fig. 1f. For the current nanocomposite, the characteristic vibration peak at 680 cm−1 was assigned to the stretching mode of MgO (in the core) and other assigned peaks for the shells were formed and were in good agreement with the literature. After conducting a comparative FTIR analysis of bare MgO-NPs, a peak located at 3040 cm−1 was assigned to the –OH stretching region. Another peak located at 731 cm−1 was appointed to the stretching mode of the Mg-O core, which slightly shifted as compared with Mg-O in the synthesized nanocomposite due to the absence of organic shells. After the FTIR conduct of the bare MgO-NPs and the confirmation of the functional groups’ presence as represented in the synthesized nanocomposite, the formation of core–shell construction was successfully indicated. The literature comparison was achieved between the FTIR data of bare FA (Mohammed 2014), HA (Reddy and Karunakaran 2013), DCA (Yang et al. 2018), 2DG (** et al. 2019), and bare MgO-NPs (Balakrishnan et al. 2020). It must be noted that the connection type between the outer organic shells and the chemical reactions on the surface of MgO-NPs was by intramolecular hydrogen bonding (weak bond) as described before, which was not present in bare FA, HA, DCA, 2DG, and bare MgO-NPs that indicated the incorporation behavior between outer layers (FA, HA, DCA, and 2DG) as indicated by a weak bond as described in recent publications (El-Batal et al. 2022). On the other hand, broadband and the change presented at 3725 cm−1 in the case of the synthesized DDM (Fig. 1f) is related to the presence of hydroxyl groups and is attributed to OH-stretching, and was changed in the case of bare MgO-NPs (3040 cm−1), which indicates the formation of intermolecular hydrogen bonding between FA, HA, DCA, 2DG, and the synthesized core MgO-NPs. The incorporation behavior was detected in our FTIR results as new peaks formed in the nanocomposite that were not present in bare MgO-NPs as a minor shifting in the bare peaks (weak physical bond; Van der Waals forces) (Uppuluri et al. 2000; Bonn and Hunger 2021).
Characterization of AF (HA-FA-Amygdaline@Fe2O3)
The XRD diffractogram of the synthesized HA-FA-Amygdaline@Fe2O3 sample showed a high-degree hematite (Fe2O3) in the core. An XRD system was conducted to study the crystal composition and state of the incorporated Fe2O3 NPs (Fig. 2a). The XRD models agree with the specific Fe2O3 original (JCPDS No. 33-0664). The unique peaks was looked at the next 2θ at 24.18°, 33.16°, 35.55°,40.69°, 49.42°, 54.19°, 57.49°, 62.19°, and 64.18° corresponding to 012, 104, 110, 113, 024, 116, 018, 214, and 300 planes, respectively, and showing its standard cubic spinel composition (Karade et al. 2019). There are no unknown crystalline phases or impurities in the Fe2O3 NPs, which represent a high concentration in the core. This matches with the unique composition of the complete Fe2O3 crystal with a rhombohedral centered hexagonal building (R3c space system) (Sharma 2017; Zeng et al. 2017; Fouad et al. 2019; Tadic et al. 2019; Liang et al. Full size image
The composition of the synthesized HA-FA-Amygdaline@Fe2O3 sample is analyzed by EDX (Fig. 2b), where the presence of O, C, N, and Fe was confirmed, where the existence of Fe, and O atoms was confirmed for the core Fe2O3 NPs. Moreover, the presence of O, C, N, was attributed to the B-17, FA, and HA multi-shell structures in the synthesized sample (Ashour et al. 2018; Abdel Maksoud et al. 2018; Maksoud et al. 2019). In order to further illustrate the structural features of the samples, elemental map**s have been carried out selectively on the synthesized HA-FA-Amygdaline@Fe2O3 and the images are depicted in Fig. 2c. It was evident from these images that the elements Fe, C, N and O existed, which agreed with the preceding EDX results. Furthermore, those elements were homogeneously distributed. From the images, it could be concluded that both Fe and O atoms were located in the same places, which confirms the core structure.
The SEM images of the synthesized HA-FA-Amygdaline@Fe2O3 are shown in Fig. 2d. The surface behavior was shown as dark layers that confirm the outer shells (B-17, FA and HA) with remarkable smooth agglomerates that could be observed due to the occupation of a large quantity of layers at the grain boundary, which could control the grain growth (Zipare et al. 2018). Also, the bright particles represented the Fe2O3 NPs in the core, which confirms the promising core–shell structure.
An HR-TEM image of the core–shell structure of the synthesized HA-FA-Amygdaline@Fe2O3 is shown in Fig. 2e. The synthesized composite possesses semi-spherical structure with diameter sizes ranging from 155.55 to 98.58 nm, with an average size of 111.95 nm. It must be noted that the condensed particles were attributed to the core Fe2O3 NPs while the faint layers corresponded to the shell layers (B-17, FA, and HA), which were entirely validated by color in map**/SEM images.
The data represented in Fig. 2f show the FTIR spectra of the synthesized HA-FA-Amygdaline@Fe2O3, and bare Fe2O3 NPs samples. For the present nanocomposite (HA-FA-Amygdaline@Fe2O3), the characteristic vibration peak at 637 cm−1 was assigned to the stretching mode of Fe–O (in the core) and was in a good agreement with the literature (Shebanova and Lazor 2003; Luo et al. 2020), and a noted peak located 726 cm−1 in the synthesized bare Fe2O3 NPs indicated a finger print for Fe–O. At the same time, a broad peak assigned at 3333 cm−1 (bare Fe2O3 NPs) was assigned to O–H group from water molecules.
In the FTIR results, the characteristic IR absorption peaks at 1608, 1691 and 1562 cm−1 were observed in the spectrum, which was assigned to folic acid due to N–H bending vibration of CONH group, C=O amide stretching of the α-carboxyl group, and the absorption band of phenyl ring, respectively (He et al. 2009). The presence of a band at 3101 cm−1 was attributed to OH and NH stretching regions. The band at 2469 cm−1 could be attributed to the stretching vibration of C−H in HA. The band at about 1691 cm−1 corresponds to the amide carbonyl and the band at 1486 cm−1 could be attributed to the stretching of COO−, which refers to the acid group of molecule HA. The absorption band at 1044 cm−1 was attributed to the linkage stretching of C−OH in HA (de Oliveira et al. 2017).
Infrared spectra of vitamin B 17 were indicated by the presence of narrow peak bands at 1859 cm−1 attributed to aldehyde and ketone C=O stretching (Thakur et al. 2019). The position of the C=O stretching indicated the hydrogen bonding and incorporation within the molecules (Nasser et al. 2021). High-intensity peak followed by peak at 2964 cm−1 and 2873 cm−1 attributed to O–H stretching (carboxylic acid) vibrations and aldehyde C–H stretching. These O–H stretching vibrations might be due to carboxylic compounds in the polymer protein matrix. Finally, the absorption bands at 1493 cm−1, 1417 cm−1, and 770 cm−1 are assigned to amide II, amide III, and amide IV (Garg et al. 2007).
After the literature comparison achieved between the FTIR data of bare FA (Mohammed 2014), HA (Reddy and Karunakaran 2013), V B17 (Jaszczak-Wilke et al. 2021), and bare Fe2O3 NPs (Azmat et al. 2020), it is worth mentioning that the connection type between the outer organic shells and the chemical reactions on the surface of Fe2O3 NPs was by intramolecular hydrogen bonding (weak bond) as described previously, which was not present in bare FA, HA, amygdalin, and bare Fe2O3 NPs that indicated the incorporation behavior between the outer layers (FA, HA, and amygdalin) as indicated by a weak bond as described in recent publications (El-Batal et al. 2022). In our FTIR results, the incorporation behavior was detected as new peaks formed in the synthesized nanocomposite and not present in bare Fe2O3 NPs as a minor shifting in the bare peaks (weak physical bond; Van der Waals forces) (Uppuluri et al. 2000; Bonn and Hunger 2021). On the other hand, broadband and the change presented at 3200 cm−1 in the case of the synthesized AF (Fig. 2f) is related to the presence of hydroxyl groups and is attributed to OH-stretching, and was changed in the case of bare Fe2O3 NPs (3333 cm−1), which indicates the formation of intermolecular hydrogen bonding between HA, FA, Amygdaline, and the synthesized core Fe2O3 NPs.
Cytotoxicity assay
After 24 h, the anti-cancer effects of both DDM and AF on BCCs (MCF-7 and MDA-MB-231) revealed an anti-proliferative activity against the cancer cell lines (Fig. 3).The IC50 of DDM was revealed at 281.9 µg/ml and 192.8 µg/ml for MCF-7 and MDA-MB-231 cells, respectively (Fig. 3a). The IC50 of AF was observed at 180 µg/ml and 184.1 µg/ml for MCF-7 and MDA-MB-231 cells, respectively (Fig. 3b).
Fig. 3
Cytotoxicity, release, cellular selectivity, and uptake of DDMPlusAF nanocomposites. a and b Cytotoxic profile of a DDM and b AF performed using MTT assay on BCCs (MCF-7 and MDA-MB-231) at different concentrations (the values are displayed as mean ± SEM carried out in triplicates from two independent experiments), c Represent the in vitro release behavior of DDMPlusAF at different pH = 3, 7, and 9 quantified using UV–vis spectrometry, d protein expression of CD44 in normal and BCCs, e representative flow cytometric chart reporting the expression pattern for CD44 in different groups, and f FR-α gene expression in BCCs determined by qRT-PCR. g Intracellular MgO and Fe2O3 uptake results in MCF-10A, MCF-7, and MDA-MB-231 cells after 24 h incubation with DDMPlusAF at IC50 doses. h Represent TEM images of DDMPlusAF uptake in MCF-10A, MCF-7, and MDA-MB-231 after 24 h incubation with DDMPlusAF at IC50 doses measured by AAS technique. Normal breast cells (MCF-10A) and breast cancer cells (MCF-7 and MDA-MB-231). Data are presented as mean ± SEM (n = 3). a1p < 0.001, a2p < 0.01 vs. untreated normal cells; b1p < 0.001, b2p < 0.01 vs. untreated cancer were considered significant
To determine nanoparticles stability, the sizes and charges of DDM and AF nanocomposites were monitored using dynamic light scattering (DLS) and zeta (ζ) potential analyses (as shown in Additional file 1: Data S1). Over 6 days dispersed in PBS plus 10% FBS, the average hydrodynamic diameter of DDM and AF remained essentially stable; nanoparticles did not aggregate. DLS measurements revealed that DDM and AF had a hydrodynamic diameter average of 352.49 nm. Furthermore, as incubation time was increased, the ζ-potential of nanoparticles was stabilized at values ranging from − 0.01 to − 3.01 mV for DDM and AF. Negative surface charges on nanoparticles were neutralized by interactions with the medium’s cationic constituents, resulting in lower negative-potential values. Notably, interactions did not result in nanoparticle aggregation even after a 6-day incubation period, indicating long-term hydrodynamic stability in a bio-relevant medium.
DDMPlusAF release
The release behavior of DDMplusAF in vitro was studied using UV–Vis at pH values of 5.5, 7, and 9 in phosphate buffer solutions (PBS) containing DMSO 0.1% and propylene glycol 0.1% to simulate the neutral environment of normal cells and acidic conditions in cancer cells to determine the pH-dependent drug-releasing properties. At pH 5.5, as shown in Fig. 3d, more than 55% of DDMplusAF is released. However, due to protonation and solubility of DDM and AF in acidic environments, the release rate of DDM at pH 7 and 9 was less than 10% and 1% DDM, respectively, in 24 h, whereas less than 5% and 1% of AF were released over 24 h at pH 7 and 9, respectively.
Cellular selectivity and uptake of DDMPlusAF
The expression levels of CD44 and FR-α were measured in normal breast cells and both cell lines of breast cancer to reveal the selectivity of DDMPlusAF (Fig. 3). In MCF-10A (normal cells) treated with DDMPlusAF, the data showed insignificant change in the levels of CD44 (Fig. 3d, e) and FR-α (Fig. 3f) as compared to untreated MCF-10A cells. When compared to MCF-10A, CD44 and FR-α expression levels were increased significantly in untreated MCF-7 (by 4.96- and 2.53-fold, respectively) and MDA (by 4.72- and 3.74-fold, respectively). However, when compared to untreated MCF-7 and MDA cells, there was a significant reduction in CD44 (Fig. 3d, e) and FR-α (Fig. 3f) expression in MCF-7 + DDMPlusAF (by 66.07 and 58.12%, respectively) and MDA + DDMPlusAF (by 67.37 and 72.76%, respectively). As a result of the HA and FA incorporation into the DDMPlusAF system, it is possible to conclude that DDMPlusAF is non-selective to normal cells and has a high affinity to CD44 and FR-α receptors that are over-expressed on breast cancer cell membranes.
Figure 3g depicts the cellular uptake and localization of DDMPlusAF in normal cells (MCF-10A) and cancer cells (MCF-7 and MDA-MB-231 cells) using AAS data. Quantitative data showed that DDM uptake was maximized by MCF-7 and MDA-MB-231 cells (7.2- and 7.6-fold, respectively) and AF was internalized by MCF-7 and MDA-MB-231 cells (5.5- and sixfold, respectively) over normal cells. These findings confirmed DDMPlusAF’s selective uptake into BCCs when compared to normal cells.
A TEM analysis was performed to visualize the internalized nanoparticles and assess their distribution in relation to subcellular compartments (Fig. 3h). In TEM images, abundant high electron density-staining nanoparticles were found inside the cells treated with DDMPlusAF, which were not displayed in DDMPlusAF untreated cells (Fig. 3h). The MCF-10A cells (normal) treated with DDMPlusAF manifested a lower uptake of nanoparticles than the cancer cells (MCF-7 and MDA-MB-231 cells). In contrast, the uptake of nanoparticles by cancer cells treated with DDMPlusAF was significantly higher, with a significant difference at p < 0.001. The uptake of DDMPlusAF particles was calculated depending on the intracellular concentration of DDMPlusAF. These values are measured against the estimated number of DDMPlusAF introduced to the MCF-7 and MDA-MB-231 cells, which mean ~ 66.5 and 84.6% of nanoparticles, respectively, from IC50 dose are more efficiently internalized than normal cells (Fig. 3h).
Cell survival and radiosensitization of DDMPlusAF
To investigate the radiosensitizing ability of DDMPlusAF, multi-MTT assays were performed on both BCCs exposed to 3 Gy-SDR or 6 Gy-FDR as illustrated in Fig. 4a. In the current study, DDMPlusAF was selected as the synergistic therapy for cancer after it is significantly declined the cell viability of both BCCs, which was confirmed through the M-MTT assay carried out on DDM, AF and DDMPlusAF along with the both doses of γ-radiation (Additional file 1: Data S2a and b).
Fig. 4
Cell survival and radiosensitizing capability of DDMPlusAF combined with different γ-radiation doses in BCCs generated using M-MTT assay at 24, 48, and 72 h. a Schematic diagram illustrates the scheme of experimental procedures for the M-MTT assay, b and c surviving fractions (SF) of MCF-7 and MDA-MB-231 cells, respectively, treated with DDMPlusAF and/or γ-radiation at 3 and 6 Gy. d and e Dose-modifying factor (DMF) curves of MCF-7 and MDA-MB-231cells, respectively. Data are represented as mean ± SEM, where the control cells are set at 85% confluence (n = 3). ap < 0.001 vs. control; bp < 0.001 vs. 3 Gy; cp < 0.001 vs. 6 Gy groups; dp < 0.001 vs. DDMPlusAF group and ep < 0.05 vs. DDMPlusAF + 3 Gy group
When cells were exposed to 3 Gy-SDR or 6 Gy-FDR, the data showed a non-significant change in survival rate between BCCs as compared to BCCs without therapy. However, DDMPlusAF therapy reduced the survival of MCF-7 cells by 43.46, 47.17, and 58.23% and by 43.94, 50.85 and 62.03% in MDA cells at 24, 48, and 72 h, respectively, compared to untreated BCCs (Fig. 4b, c).
On the other hand, compared to DDMPlusAF group, a significant elevation was observed in the survival of MCF-7 + 3 Gy treated cells by 1.84-, 1.89-, and 2.39-fold, MCF-7 + 6 Gy treated cells by 1.68-, 1.84-, and 2.39-fold, MDA + 3 Gy exposed cells by 1.78-, 2.03-, and 2.59-fold, and MDA + 6 Gy exposed cells by 1.69-, 1.87-, and 2.39-fold at 24, 48, and 72 h, respectively (Fig. 4b, c).
Furthermore, the BCCs survival rate was significantly decreased in MCF-7 + DDMPlusAF + 3 Gy group to 41.79, 64.11, and 79.40%, and in the MDA + DDMPlusAF + 3 Gy group to 36.26, 74.52, and 77.07% at 24, 48, and 72 h, respectively, when compared to the DDMPlusAF group. Additionally, the DDMPlusAF + 6 Gy group induced a significant decrease in the survival fraction of MCF-7 to 83.11, 84.08, and 83.74%, and in MDA cells to 86.09, 80.16, and 82.44% at 24, 48, and 72 h, respectively, when compared to DDMPlusAF group (Fig. 4b, c).
Moreover, the survival rate in the DDMPlusAF + 3 Gy group revealed a significant decline in MCF-7 cells to 66.10, 81.04, and 91.39%, and in MDA cells to 64.27, 87.45, and 91.13 compared to BCCs exposed to 3 Gy at 24, 48, and 72 h, respectively. In addition, when compared to BCCs exposed to 6 Gy at 24, 48, and 72 h, the growth inhibition rate in the DDMPlusAF + 6 Gy group was 89.97, 91.33, and 93.21% for MCF-7 cells and 91.79, 89.42, and 92.66% for MDA cells (Fig. 4a, b). Furthermore, when DDMPlusAF + 6 Gy was compared to DDMPlusAF + 3 Gy, MCF-7 cells survived at 71.01, 55.65, and 21.07%, respectively, while MDA cells survived at 78.19, 22.12, and 23.43% at 24 h, 48 h, and 72 h, respectively. According to the above survival data of all groups and time intervals, it was revealed that DDMPlusAF + 6 Gy after 24 h has the best anti-cancer effect (Fig. 4b, c).
Figure 4d, e) depicts the dose modifying factor (DMF) data for all groups, whereas, at 24 h, the dose–response rates of 3 Gy and 6 Gy were the same on BCCs. But after DDMPlusAF therapy, the dose–response rates of the DDMPlusAF + 3 Gy and DDMPlusAF + 6 Gy groups were elevated compared to each therapy alone. Furthermore, the DDMPlusAF + 6 Gy group had a higher dose–response rate than the DDMPlusAF + 3 Gy group. These results showed that DDMPlusAF induced a greater radiosensitizing modified effect with 6 Gy than with DDMPlusAF + 3 Gy; thus, the 6 Gy at 24 h was chosen for further investigations (Fig. 4d, e).
Cell cycle arrest and apoptosis analysis
Cell cycle distribution and cell apoptosis were measured using flow cytometry to assess DDMPlusAF’s role as an anti-cancer and radiosensitizer to 6 Gy in BCCs. The cell cycle analysis of untreated BCCs (MCF-7 or MDA cells) showed an arrest at the G1 phase. When compared to MCF-7 cells, the MCF-7 + 6 Gy group displayed an arrest at the S phase (Fig. 5a), whereas the MDA + 6 Gy group showed a higher proportion in the G1 phase, comparable to MDA cells (Fig. 5b). Nevertheless, after DDMPlusAF therapy, a remarkable elevation in G2/M and pre-G1 phases was observed in both cell lines when compared to groups of BCCs and 6 Gy of each BCC. Furthermore, when compared to the untreated BCCs and BCCs exposed to 6 Gy of each cell line, the combination group DDMPlusAF + 6 Gy implied a higher proportion in G2/M and pre-G1 phases and a lower proportion in G1 and S phases in both cell lines.
Fig. 5
Analysis of cell cycle distribution in DDMPlusAF and/or 6 Gy treated BCCs. Cell cycle charts of a distribution of MCF7 cells through the cell cycle phases and a representative histogram for the cell arrest percentage at various checkpoints, and b distribution of MDA-MB-321 cells through the cell cycle phases and a representative histogram for the cell arrest percentage at various checkpoints. Data are represented as mean ± SEM, a1p < 0.001, a2p < 0.01, a3p < 0.05 vs. Control group; b1p < 0.001, b2p < 0.01, b3p < 0.05 vs. DDMPlusAF group; c1p < 0.001, c2p < 0.01, c3p < 0.05 vs. 6 Gy group. Control group is MCF-7 or MDA cells
The analysis of apoptotic cells revealed that the DDMPlusAF group had a higher percentage of apoptotic cells in both cell lines than the corresponding untreated BCCs (Fig. 6). Furthermore, when compared to the BCCs and BCCs + 6 Gy groups of each type, the combination group DDMPlusAF + 6 Gy has a higher percentage of apoptotic cells in both cell lines. Moreover, DDMPlusAF + 6 Gy induced an increase in necrotic cell percentage in both cell lines when compared to BCCs, 6 Gy, and DDMPlusAF of each BCC type.
Fig. 6
Detection of apoptosis in DDMPlusAF and/or 6 Gy treated BCCs. Representative dot-plot images of the Annexin-V-FITC and PI performed on BCCs treated with DDMPlusAF and/or 6 Gy. a DDMPlusAF and 6 Gy induced apoptosis and necrosis in MCF-7 cells, and b DDMPlusAF and 6 Gy induced apoptosis and necrosis in MDA-MB-231 cells. The overall percentage of dead cells comprises the total apoptotic cells (early and late) as well as the necrotic cells. Data are represented as mean ± SEM, a1p < 0.001, a2p < 0.01, a3p < 0.05 vs. Control group; b1p < 0.001, b2p < 0.01, b3p < 0.05 vs. DDMPlusAF group; c1p < 0.001, c2p < 0.01, c3p < 0.05 vs. 6 Gy group. Control group is MCF-7 or MDA cells
Modulatory effect of DDMPlusAF on tumor-promoting factors and metabolic reprogramming
This study is designed to target the tumor-promoting factors (TPF) and metabolic reprogramming via the combination of DDMPlusAF with radiotherapy at 6 Gy in BC therapy. This was accomplished by evaluating the biochemical mediators constitute a tumor-promoting milieu (HIF-1α, TNF-α, IL-10, p53, PPAR-α, and PRMT-1) (Fig. 7) compared to the glycolytic metabolism (glucose, HK, PDH, lactate, and ATP) (Fig. 8) and signaling effectors (protein expression of AKT, AMPK, SIRT-1, TGF-β, PGC-1α, and gene expression of ERR-α) (Fig. 9).
Fig. 7
Modulatory effect of DDMPlusAF and/or 6 Gy on the biochemical mediators constitute TPF in BCCs. a HIF-1α, b TNF-α, c p53, d PPAR-α, e IL-10, and f PRMT-1. All group values are represented as mean ± SEM. a1p < 0.001, a2p < 0.01, a3p < 0.05 vs. control; b1p < 0.001, b2p < 0.01, b3p < 0.05 vs. DDMPlusAF group; c1p < 0.001, c3p < 0.05 vs. 6 Gy group. Blue columns denote MCF-7 cells and red columns stand for MDA-MB-231 cells
Modulatory effect of DDMPlusAF and/or 6 Gy on the glycolytic metabolism of BCCs. a Glucose, b HK, c PDH, d lactate, and e ATP. All group values are represented as mean ± SEM. a1p < 0.001, a2p < 0.01, a3p < 0.05 vs. control; b1p < 0.001, b2p < 0.01, b3p < 0.05 vs. DDMPlusAF group; c1p < 0.001, c3p < 0.05 vs. 6 Gy group. Blue columns denote MCF-7 cells and red columns stand for MDA-MB-231 cells
Regulatory role of DDMPlusAF and/or 6 Gy on signaling effectors implicated in metabolic reprogramming of BCCs. The protein expression of a AKT, b AMPK, c SIRT-1, d TGF-β, e PGC-1α were detected by western blotting (β-actin, as housekee** protein), f gene expression of ERR-α via RT-PCR, and g, h representative western blot analysis, SDS-PAGE of MCF-7 and MDA, respectively. All group values are represented as mean ± SEM. a1p < 0.001, a2p < 0.01, a3p < 0.05 vs. control; b1p < 0.001, b2p < 0.01, b3p < 0.05 vs. DDMPlusAF group; c1p < 0.001, c3p < 0.05 vs. 6 Gy group. Blue columns denote MCF-7 cells and red columns stand for MDA-MB-231 cells
Biochemical mediators constitute a tumor-promoting milieu
As demonstrated in Fig. 7, the DDMPlusAF group showed a significant reduction in the level of HIF-1α (31.18% for MCF-7 and 44.70% for MDA), TNF-α (60.20% for MCF-7 and 52.84% for MDA) (Fig. 7a, b), and PRMT-1 (55.21% for MCF-7 and 37.6% for MDA) (Fig. 7f), associated with a significant elevation in p53 (1.79-fold for MCF-7 and 2.09-fold for MDA), PPAR-α (2.71-fold for MCF-7 and 2.89-fold for MDA), and IL-10 (3.18-fold MCF-7 and 3.68-fold MDA) levels (Fig. 7c–e) when compared to the control BCCs. Exposure to 6 Gy induced a significant decrease in the levels of HIF-1α (22.19% for MCF-7 and 39.79% for MDA) and TNF-α (54.19% for MCF-7 and 47.52% for MDA) (Fig. 7a, b) and PRMT-1 (47.81% for MCF-7 and 56.8% for MDA), associated with a significant increase of P53 (1.81-fold MCF-7 and 1.46-fold MDA), PPAR-α (2.61-fold for MCF-7 and 2.49-fold for MDA) and IL-10 (3.26-fold for MCF-7 and 3.24-fold for MDA) levels (Fig. 7c–e) when compared to the untreated BCCs. In DDMPlusAF + 6 Gy group, the data display a significant diminish in the levels of HIF-1α (33.15% for MCF-7 and 55.39% for MDA) and TNF-α (55.15% for MCF-7 and 56.37% for MDA) (Fig. 7a, b) and PRMT-1 (72.92% for MCF-7 and 75.2% for MDA), associated with a significant elevation of p53 (1.95-fold for MCF-7 and 2.02-fold for MDA), PPAR-α (2.77-fold for MCF-7 and 3.07-fold for MDA) and IL-10 (3.47-fold for MCF-7 and 5.04-fold for MDA) levels (Fig. 7c–e) when compared to BCCs without therapy. It was observed that the data of the MDA + DDMPlusAF + 6 Gy group reveal a significant decrease in HIF-1α (25.91%) (Fig. 7a), a considerable elevation in p53 (1.38-fold) (Fig. 7c) and IL-10 (1.56-fold) levels (Fig. 7e) as compared with the MDA + 6 Gy group; as well as markedly raised IL-10 level (1.37-fold) (Fig. 7e) when compared with the MDA + DDMPlusAF set. Conversely, the combination of DDMPlusAF and 6 Gy caused a significant diminish in PRMT-1 level in MCF-7 (39.53 and 48.10%, respectively) and MDA (60.26 and 42.59%, respectively) cells as compared with DDMPlusAF and 6 Gy groups, respectively, of the both cell lines (Fig. 7f).
Glycolytic metabolism
In Fig. 8, the mediators of glycolytic pathway are discerned, when MCF-7 cells were treated with DDMPlusAF or 6 Gy, there was a significant diminution in glucose (31.67 and 25.39%) (Fig. 8a), HK (61.28 and 32.62%) (Fig. 8b), PDH (65.71 and 72.11%) (Fig. 8c), lactate (55.89 and 49.42%) (Fig. 8d), and ATP (49.18 and 42.81%) (Fig. 8e). In addition, when compared to the DDMPlusAF group, 6 Gy treated BCCs showed a significant increase in HK (1.74-fold) in both cell lines. While, the results of DDMPlusAF + 6 Gy manifested a significant reduction in the levels of glucose (36.67%) as compared with MCF-7 group, HK (51.83 and 28.51%), lactate (66.88 and 34.53%) as compared to MCF-7 and 6 Gy groups, respectively, and PDH (76.70 and 32.05%) as compared with MCF-7 and DDMPlusAF groups, respectively, as well as ATP (69.60, 40.18, and 46.84%) as compared to MCF-7, DDMPlusAF, and 6 Gy groups, respectively. In MDA cell line, the data of DDMPlusAF or 6 Gy groups detected a significant decrease in glucose (56.19 and 33.97%) (Fig. 8a), HK (54.77 and 32.41%) (Fig. 8b), PDH (63.75 and 52.44%) (Fig. 8c), lactate (70.45 and 66.77%) (Fig. 8d), and ATP (53.69 and 40.85%) levels (Fig. 8e), respectively, as compared to the untreated MDA cells. Moreover, when compared to the DDMPlusAF group, 6 Gy showed a significant increment in glucose (1.51-fold) and HK (1.49-fold) levels. When compared to MDA and 6 Gy groups, the combination group of DDMPlusAF and 6 Gy showed a significant decrement in glucose (58.92 and 37.79%), ATP (67.86 and 44.25%); and in HK (48.55%), PDH (60.92%), and lactate (76.34%) levels, when compared to the MDA group set (Fig. 8).
Signaling effectors implicated in oncogenesis and metabolic reprogramming of BCCs
The data illustrated in Fig. 9a–f revealed a profound down-regulation in the protein expression of MCF-7 AKT by 44.55 and 51.81% (Fig. 9a), AMPK by 66.05 and 63.89% (Fig. 9b), SIRT-1 by 62.02 and 61.03% (Fig. 9c), TGF-β by 45.28 and 42.45% (Fig. 9d), and PGC-1α by 55.44 and 59.43% (Fig. 9e) paralleled by a substantial decline in the gene expression of ERR-α by 65.69 and 62.74% (Fig. 9f), respectively, in DDMPlusAF and 6 Gy groups, respectively, when compared to the untreated MCF-7 group. Similarly, a pronounced curtailment in the protein expression of AKT by 55 and 62%, AMPK by 52.94 and 46.20%, SIRT-1 by 76.24 and 73.28%, TGF-β by 53.92 and 58.99%, and PGC-1α by 40.38 and 34.61% coupled with a significantly lowered gene expression of ERR-α by 48.62 and 33.94% in DDMPlusAF and 6 Gy groups as compared to the control MDA group (Fig. 9a–f).
In DDMPlusAF + 6 Gy of MCF-7 treated cells, the results showed a significant reduction in the protein expression of AKT by 69.30, 44.64, and 36.30%, AMPK by 79.63, 40.00, and 43.59%, SIRT-1 by 75.66, 35.89, and 40.00%, TGF-β by 65.09, 36.21, and 39.34%, and PGC-1α by 72.28, 37.78, and 31.66%, as well as the gene expression of ERR-α by 82.35, 48.57, and 52.63%, respectively, when compared to MCF-7, DDMPlusAF, and 6 Gy groups, respectively (Fig. 9a–f). Additionally, when compared to MDA, DDMPlusAF, and 6 Gy groups, the MDA + DDMPlusAF + 6 Gy group displayed a significant diminution in the protein expression of AKT by 74.00, 42.21, and 31.58%, AMPK by 69.61, 35.42, and 43.50%, and PGC-1α by 68.36, 64.93, and 51.62%, respectively (Fig. 9). Moreover, as compared with MDA group, the protein expression of SIRT-1 and TGF-β were markedly lowered by 82.50 and 65.69%, respectively, while the gene expression of ERR-α revealed a significant decline by 35.24 and 29.21%, when compared to MDA and 6 Gy groups, respectively (Fig. 9a–f).
Discussion
The CD44 and FR-α expression data revealed that the selectivity-mediated cellular uptake of DDMPlusAF nanocomposites was reduced in normal breast cells (MCF-10A) and maximized in BCCs. Our data revealed that the incorporation of surface annex receptor-mediated uptake (HA and FA), which enabled the optimum tumor targeting, augmented the selective cytotoxicity of DDMPlusAF towards BCCs with no affinity for normal breast cells. This uptake indicates HA/FA-mediated endocytosis by BCCs. Therefore, DDM and AF can enter cancer cells through binding to a specific receptors CD44 and FR-α, which are over-expressed on BCCs via HA/FA, respectively (Liu et al. 2019). The results of pH-responsive release of DDMPlusAF were shown to be performed in acidic conditions (pH = 5.5) of cancer rather than normal cells, and this result supported with the data reported by Guo et al. (2017) and Jurczyk et al. (2021).
Radiotherapy has been harnessed for over a century to treat patients with cancer, largely based on the rationale that rapidly proliferating cancer cells are more sensitive than normal cells for the DNA damage response, but in terms of the consequences of radiation-induced tumor cell death and various signaling pathways involved in sensitivity, resistance, and further molecular sensors that modify the tumor response to radiation (Baskar et al. 2014). Furthermore, it was found that the alterations in the glycolytic metabolism were shown to contribute to the declining radiotherapy effect. Additionally, radiotherapy effects primarily depend on glucose metabolism, while the mitochondrial metabolic alterations can be involved in this process as well (Tang et al. 2018). Therefore, targeting of the metabolic enzymes, such as glucose transporters, HK, pyruvate kinase M2, lactate dehydrogenase A, PDK, fatty acid synthase, and glutaminase, can enhance the efficacy of chemotherapy or radiotherapy, as observed, for example with 2-DG and DCA when combined with chemotherapy or radiotherapy (Zhao et al. 2013).
The anti-cancer effect of DDMPlusAF with γ-radiation was demonstrated by the reduction of both BCCs’ viability through cell cycle arrest at G2/M and pre-G1 phases, which generates apoptotic cell death compared to untreated cancer cell lines. Additionally, this could be attributed to their modulatory effects that are displayed on TME-associated TPF and mediators, glycolytic pathways, and signaling molecules as revealed in the current study. Noteworthy, the innovative DDM and AF core–shell nanocomposites have numerous attractive characteristics. DDM core–shell induced an anti-cancer effect through its components such as the ability of 2-DG, a stable glucose analogue, to inhibit glycolysis due to the formation and intracellular accumulation of 2-deoxy-d-glucose-6-phosphate (2-DG6P), inhibiting the function of HK and glucose-6-phosphate isomerase, and inducing apoptotic cell death (Pajak et al. 2019). Moreover, DCA reverses the Warburg effect in human tumor cells by inhibiting PDK, re-activating PDH and OXPHOS, as well as decreasing pyruvate and lactate levels, leading to decreased expression of HIF-1α. As a consequence of OXPHOS stimulation, DCA increases reactive oxygen species (ROS) production by the mitochondrial respiratory chain and induces other downstream changes in mitochondrial function, resulting in tumor cell-selective apoptosis, decreased cancer cell proliferation, and increased host survival (James et al. 2017). Furthermore, AF core–shell induced an anti-cancer effect via amygdalin, which inhibits TNF-α levels, AKT-mTOR, and TGF-β pathways, while increasing the levels of P53, Bax, cytochrome c, caspase-3, and finally cell cycle arrest at G2/M (Liczbiński and Bukowska 2018; El-Desouky et al. 2020). This inhibitory effect of AF on TNF-α could explain why aerobic glycolysis and ATP production in BCCs are declining. In support of this notion, the study of Vaughan et al. (2013) reported that curcumin, as anti-inflammatory agent, suppresses TNF-α and, as a result, reduces aerobic glycolysis and ATP production in MCF-7 cells. Furthermore, Liu et al. (2016) elucidated that inhibiting HIF-1α and TNF-α prevents metabolic reprogramming in cell models of dextran sulfate sodium (DSS)-induced colitis in mice, which is used to treat this disease. Moreover, the studies of Ahamed et al. (2013) and Behzadi et al. (2019) demonstrated that MgO and Fe2O3 nanoparticles induce apoptosis in cancer cells through increasing the load of intracellular ROS. This elevation induced an up-regulation of p53 level in cancer cells (Ahamed et al. 2013; Perillo et al. 2020). In addition, it was found that the p53 protein induces a decrease in glycolytic pathway, and overall levels of intracellular ROS (Puzio-Kuter 2011).
Moreover, to maintain cancer cell proliferation and survival in the hypoxic microenvironment, an interplay between HIF-1 and a variety of oncogenes such as p53, AMPK, and AKT signaling pathways has been observed to contribute to the metabolic reprogramming of cancer cells and to control mitochondrial electron transport chain functioning and energy production (Moldogazieva et al. 2020). Additionally, it was found that hypoxia up-regulates PRMT-1 (Wrzesinski and Fey 2018). On the other hand, Lee and Park (2011) demonstrated that reduction of HIF-1α accompanied by decreased AMPK activity. Furthermore, it was demonstrated that p53 up-regulation decreased the stability of PGC-1α via the ubiquitin proteasome pathway, which was mediated by AKT inhibition and glycogen synthase kinase (GSK-3β) activation (Deng et al. 2020). Moreover, increasing p53 activity could reduce the expression level of SIRT-1 through a negative feedback loop (Deng 2009). According to Tan et al. (2016), the down-regulation of AMPK and SIRT-1 signaling molecules led to the suppression of PGC-1α. As a result, the PGC-1α/ERR-α axis and its downstream promote glycolysis and OXPHOS in cancer (Tan et al. 2016) were inhibited, as revealed in our data. The elevation of PPAR-α level observed in this study could be attributed to 2DG, which mimics the dissociative effect of glucose-6-phosphate on the HK/VDAC (voltage-dependent anion channel) complex (Vamecq et al. 2012); Whereas, it was found that the activation of PPAR-α was attributed to HK and VDAC dissociation when fenofibrate, a PPAR-α agonist, was administered to cell lines and a mouse model of oral cancer (Antonosante et al. 2018). PPAR-α activation has anti-cancer effects as a possible trigger of ineffective tumor metabolism, blocking fatty acid synthase (FAS) pathway, which is one of cancer cells metabolic peculiarities along with aerobic glycolysis, inhibiting AKT phosphorylation, and imparting an anti-inflammatory properties (Grabacka and Reiss 2008; Antonosante et al. 2018). This anti-inflammatory effect of PPAR-α activation is related to an elevation of IL-10 and a reduction in TNF-α expression (Cao et al. 2014). Most importantly, it was found that the increase of IL-10 inhibits glucose uptake and glycolytic flux by regulating the glycolytic enzymes (Ip et al. 2017).
Conclusions
DDMPlusAF is a combinatorial targeted anti-cancer platform with multifunctional effects that induces cell cycle arrest at G2/M and pre-G1 phases and generates apoptotic cell death in both BCC lines. Its constituents, which include 2DG (hexokinase inhibitor), DCA (PDK inhibitor), and amygdalin, suppress the aerobic glycolytic pathway and modulate TPF mediators and signaling effectors, are responsible for this effect. Specifically, through a significant decrease in glucose, HK, PDH, lactate, and ATP, concurrent with a significant reduction in protein expression of AKT, AMPK, SIRT-1, TGF-β, and PGC-1α, as well as the gene expression of ERR-α. Moreover, a significant reduction in HIF-1α, TNF-α and PRMT-1 was associated with a significant elevation in IL-10, P53, and PPAR-α (Fig. 10). Interestingly, the DDMPlusAF augmented the radiosensitivity of MCF-7 and MDA-MB-231 cell lines. Collectively, these effects of DDMPlusAF in combination with radiotherapy support its potential implication in theranostic applications for breast cancer therapy.
Fig. 10
Graphical summary. This graphical representation illustrates the modulatory effect of DDMPlusAF in combination with radiotherapy on BCCs through its components as 2DG (hexokinase inhibitor), DCA (PDK inhibitor), and amygdalin associated with exposure to 6 Gy-FDR
MgO nanoparticles (MgO-NPs) were synthesized following the technique mentioned by Diana et al. (2021) with slight modifications. Briefly, urea was dissolved into an aqueous solution of magnesium nitrate (0.25 M) under continuous stirring at 75 °C until gel creation. After that, MgO-NPs were synthesized by placing the gel at 600 °C in a muffle furnace for 3.5 h. Finally, the prepared MgO-NPs were rinsed with de-ionized water (D.I.W) and dehydrated at 75 °C for 3 h, as shown in Additional file 1: Data S3a-1.
Step two: preparation of 2DG@DCA@MgO
This unique composite construction was developed by a manageable impregnation process. After conducting water bath sonication for 60 min, the prepared MgO-NPs from step one were dispersed in 100 ml ethanol. The aqueous solutions of previously prepared DCA and 2DG (10 mM) were then added to the dispersion after 3 h of continuous stirring at room temperature (24 °C). As shown in Additional file 1: Data S3a-2, the developed particles were settled, collected, cleaned, and dehydrated.
Step three: incorporation of 2DG@DCA@MgO with HA and FA
The prepared nanocomposite structure from step two was dispersed in D.I.W for 40 min using water bath sonication. The solution was then mixed with 20 mM aqueous solutions of HA and FA, which were then sonicated for 45 min. The mixture was then stirred continuously for 3 h. Finally, the powder was obtained using centrifugation and dehydrated at 85 °C for 2 h (see in Additional file 1: Data S3a-3).
Synthesis of AF
Step one: preparation of Fe2O3 nanoparticles
Fe2O3 NPs were prepared according to the method described by Sankadiya et al. (2016) with minor modification. Firstly, 5.40 g of FeCl3. 6H2O was dissolved in (100 ml) D.I.W. using magnetic stirrer at ambient temperature for 15 min. Then, drop-by-drop, NH4 OH solution (15%) was added into the above-mentioned solution to make reaction pH = 8. The reaction was then stirred for 2 h at ambient temperature in the stirrer. The precipitate was then collected using a high-speed centrifuge running at 5000 rpm for 20 min. The formed precipitate was then washed several times using D.I.W. The purified precipitate was then dried in vacuum oven at 80 °C for 8 h. Finally, the dried powder was then annealed at 200 °C for 3 h as shown in Additional file 1: Data S3b-1.
Step two: preparation of Amygdaline@Fe2O3 and its incorporation with HA and FA
The synthesized Fe2O3 NPs (250 mg) prepared from step one were dispersed in 100 ml D.I.W. using sonication for 30 min. Amygdaline (B 17) was then poured into the above dispersion under constant stirring at room temperature. Following that, FA-HA (250 mg) was added into the above mixture under constant stirring for 2 h. The prepared powder was then collected, washed with D.I.W., and dried at 80 °C for 2 h as presented in the Additional file 1: Data S3b-2.
Characterization of DDM and AF
Firstly, the stoichiometry of the synthesized nanocomposite samples is examined by employing the energy- dispersive X-ray spectra (EDX) (JEOL JSM-5600 LV, Japan). To confirm the formation of the exact sample with detected functional groups, Fourier transform infrared (FTIR) spectroscopy (NICOLET iS10 model instrument) is conducted over a wide range (400–4000 cm−1). The crystal structure of the nanocomposite samples was investigated using X-ray diffraction technique (XRD; Shimadzu XRD-6000). XRD patterns are obtained in the range of 2θ from 17° to 90° at room temperature. Cu Kα is used as a radiation source with a wavelength λ = 0.15408 nm, a scan rate of 0.8°/min, an operation voltage of 50 kV, and a current of 40 mA (Belavi et al. 2012; Reheem et al. 2016). Information on the surface morphology of the nanocomposite samples’ particles is obtained using scanning electron microscopy (SEM) (JEOL JSM-5600 LV, Japan). Finally, the shape and size of the synthesized nanocomposite samples were obtained by high resolution transmission electron microscopy (HR-TEM) (JEOL JSM-5600 LV, Japan).
Stability of DDM and AF
To determine the stability of both nanocomposites DDM and AF, the charges and sizes were measured through the incubation of DDMPlusAF with phosphate buffer solutions (PBS) and 10% fetal bovine serum (FBS; pH 7.4) at body temperature (37 °C) using dynamic light scattering (DLS) and determining zeta (ζ) potential over 6 days (Angelopoulou et al. 2019).
Cell lines and cell culture
The breast cell lines used in this investigation were purchased from the Cell Culture Department, VACSERA (Cairo, Egypt). Normal human breast cells (MCF-10A), as well as human MCF-7 (luminal A) and MDA-MB-231 (Triple negative B) BCCs, were cultured in DMEM (Dulbecco's Modified Eagle Medium) supplemented with penicillin (100 U/ml), streptomycin (100 mg/ml), and 10% FBS (fetal bovine serum) in a 5% CO2 humidified chamber at 37 °C.
Cytotoxicity assay
MTT (3-(4,5-dimethylthiazol-2yl)-2,5-diphenyltetrozolium bromide) (Sigma-Aldrich, USA) assay on both MCF-7 and MDA-MB-231 cell lines was used to investigate the cytotoxic effect of DDM and AF, as described by Van de Loosdrecht et al. (1994). DDM and AF were dissolved in dimethyl sulfoxide (DMSO) and propylene glycol (Sigma-Aldrich, USA), respectively. The stocks were then diluted with a culture medium to the indicated concentration for treatment before usage, and the final concentration of DMSO and propylene glycol in each well was 0. 1% (V/V). Cells that were treated with the vehicle only, were kept as the control group. Briefly, in the 96-well tissue culture plate, cells were inoculated with 1 × 105 cells/ml (100 μl/well) and incubated at 37 °C for 24 h to develop a complete monolayer sheet. The growth medium was decanted from 96-well plates after a confluent sheet of cells was formed; the cell monolayer was washed twice with wash media. Twofold dilutions to both DDM and AF were made in RPMI medium with 2% serum (maintenance medium). Then, 0.1 ml of each dilution was tested in different wells leaving 3 wells as control, receiving only maintenance medium. The plate was incubated at 37 °C and examined. Cells were checked for any physical signs of toxicity, e.g., partial or complete loss of the monolayer, rounding, shrinkage, or cell granulation. A MTT solution was prepared (5 mg/ml in PBS), and after that, 20 μl of MTT solution was added to each well. Place on a shaking table at 150 rpm for 5 min to thoroughly mix the MTT into the medium. Incubate (37 °C, 5% CO2) for 1–5 h to allow the MTT to be metabolized. Dump off the media and then resuspend formazan (MTT metabolic product) in 200 μl of DMSO. Place on a shaking table at 150 rpm for 5 min to thoroughly mix the formazan into the solvent. Read optical density at 560 nm and subtract background at 620 nm. Optical densities should be directly correlated with cell quantities. Then, the half-maximal inhibitory concentration (IC50) was calculated. The cell morphology was recorded using a light inverted microscope fitted with a digital camera (Nikon, Japan). We performed all experiments in triplicate.
Release of DDM and AF in vitro
To investigate the release of DDM and AF, suspensions of each were exposed at 37 °C conditions to pH 5.5, 7, and 9. The particles were collected at predetermined time intervals using an external magnet (1.3 Tesla), and the supernatant was saved for examination after 24 h of incubation. The released proportions of MgO and Fe2O3 were quantified using UV–Vis at absorbance of 487 nm and 562 nm, respectively.
Cellular selectivity and uptake of DDMPlusAF
Normal breast cells (MCF-10A) and BCCs (MCF-7 and MDA-MB-231) were seeded in 24-well plates with round coverslips at a density of 2 × 104 cells/well. The next day, cells were incubated with medium containing an IC50 dose of DDM and an IC50 dose of AF. After 24 h incubation, the cells were washed three times with PBS and divided into four parts to perform four methods. The first and second methods were used to investigate the cellular selectivity of DDMPlusAF, which was accomplished by measuring CD44 expression by flow cytometric analysis using an FITC-conjugated anti-CD44 (1:400, Cat. No# YKIX337.8, eBioscience) incubated with cells for 30 min at 4 °C, and measuring of FR-α expression by qRT-PCR as described in real-time PCR part.
The third and fourth methods were performed to investigate cellular uptake of DDMPlusAF, which was done by estimating MgO and Fe2O3 concentration in normal and cancer cells by an atomic absorption spectrophotometer (AAS) and imaging of DDMPlusAF in normal and cancer cells using transmission electron microscopy (TEM), respectively.
The AAS model (AI-1200) was used with an air-acetylene burner (slot length, 11 cm). Instrumental settings were as follows: Wavelength [MgO = 285.2 nm, Fe2O3 = 248.3 (Najim 2017)], lamp current (5 mA), slit width (0.2 nm), air-flow (1.8 L/min), ignition-flow (2.4 L /min). A standard solution of MgO and Fe2O3 was prepared immediately by serial dilution of a 1000 mg/L stock solution (Scharlau Chemie) with de-ionized water prior to use. After 24 h incubation, the cells were washed three times with PBS, then centrifugation was carried out at 3000 rpm for 5 min and the supernatant was aspirated by using Pasteur pipette into another plain bottle. Supernatant and pellet cell samples were diluted with de-ionized water and homogenized before determination of MgO and Fe2O3 concentrations (Planeta et al. 2021).
In brief, the imaging of DDMPlusAF by TEM was performed via fixation of cells in 2.5% glutaraldehyde, at 0.1 M Phosphate Buffer, pH 7.4 (Electron Microscopy Sciences, Hatfield, PA) for 1 h at room temperature. Cells were then scraped off the plates, centrifuged at a low speed, and suspended in 2.5% glutaraldehyde. Samples were further processed at the Egyptian atomic energy authority by post-fixation in 1% osmium tetroxide, rinsing in distilled water, and dehydration through a graded series of acetone. At the end, samples were embedded in epoxy resin and cut into 70 nm sections that were then analyzed and photographed by JEOL 100CXII electron microscope (Janic et al. 2018).
Irradiation
All the irradiated groups of MCF-7 and MDA-MB-231 culture cell lines were irradiated at 85% confluence with a Canadian gamma cell-40, (137Cs) at the NCRRT (Cairo, Egypt) as fractioned doses, each of 3 Gy with a dose rate of 0.012 Gy/s. The dosimetry was used for all the experiments to ensure uniformity of dose and dose rate delivered using a Fricke reference standard dosimeter ISO/ASTM E 51026 (2015).
Multi-MTT assay
A multiple-MTT (M-MTT) assay was performed to measure the BCCs radiosensitivity of nano-core–shell composites DDMPlusAF at 3 Gy (single dose radiotherapy; SDR) and 6 Gy (fractionated dose radiotherapy; FDR) after 24, 48, and 72 h from exposure to γ-rays according to the method of Buch et al. (2012) as illustrated in Fig. 4a. Briefly, the cells incubated in 96-well plates for 24 h (2 × 103 cells per well) before being supplemented with 100 μl of MTT (3-(4,5-dimethylthiazol-2-yl)-2, 5-diphenyltetrazolium bromide) reagent (5 mg/ml in PBS, 20 µl/well) to each well and incubated for 30 min at 37 °C. Thereafter, MTT solution was removed. After the addition of 180 μl of DMSO the plates were incubated for 15 min at 37 °C to dissolve the formazan crystals. Eventually, the absorbance of each well was measured at 570 nm using an ELISA plate reader (BioTeck, Bad Friedrichshall, Germany). Following the conduction of proliferation/inhibition assays, the survival curves were calculated and utilized to obtain the Dose-Modifying Factor (DMF) calculated at the iso-effect of survival fraction (SF) = 50% with radiation treatment alone respect to combined treatments (Minafra et al. 2019).
Cell culture models
In the current study, the cultures of each MCF-7 and MDA-MB-231 cell lines were divided into four groups as following:
I.
MCF-7 cell line model; MCF-7 group: untreated MCF-7cells used as control, MCF-7 + DDMPlusAF group: MCF-7 cells treated with DDMPlusAF, MCF-7 + 6 Gy group: MCF-7 cells treated with γ-rays (6 Gy-FDR) exposure, and MCF-7 + DDMPlusAF + 6 Gy group: MCF-7 cells treated with DDMPlusAF and exposed to γ-rays 6 Gy (FDR).
II.
MDA cell line model; MDA group: untreated MDA-MB-231 cells used as control, MDA + DDMPlusAF group: MDA cells treated with DDMPlusAF, MDA + 6 Gy group: MDA cells treated with γ-rays (6 Gy-FDR) exposure, and MDA + DDMPlusAF + 6 Gy group: MDA cells treated with DDMPlusAF and exposed to γ-rays 6 Gy (FDR).
The models start with the addition of DDMPlusAF therapy to both cell lines of BCCs, then exposed to 6 Gy-FDR (3 Gy/day for two successive days) post 24 h of DDMPlusAF therapy. Then, after 24 h incubation post last dose of radiotherapy, BCCs were harvested for the biochemical investigation of anti-cancer effect of DDMPlusAF.
Flow cytometric analysis of the cell cycle and apoptosis
For all groups of both MCF-7 and MDA-MB-231 cell lines, after 24 h incubation post the last dose of radiotherapy, the 3 × 105 cells/well were harvested with trypsin, washed twice in ice-cold PBS, and fixed with 70% ethanol at 4 °C overnight. Afterwards, the cells washed with PBS and collected by centrifugation, then stained by propidium-iodide (PI) (50 µg/ml) for cell cycle analysis (Cat. No# ab139418) and using an Annexin-V-FITC Kit (Beckman Coulter, Marseille, France) for measurement of apoptosis. Staining was assessed in a FACSCanto-II flow cytometer, followed by analysis using BD Accuri-C6 Plus software (Biosciences, CA, USA) (Kojima et al. 2018).
Tumor-promoting factors (TPF) and metabolic reprogramming measurements
The levels of tumor suppressor p53, tumor necrosis factor alpha (TNF-α), interleukin 10 (IL-10), HIF-1α, and ATP were determined by using enzyme-linked immunosorbent assays (ELISA) kits purchased from Sigma-Aldrich, Cat. No# RAB0500, RAB0476, RAB0244, RAB1057, and MAK190, respectively, following the manufacturers’ instructions. Additionally, PRMT-1 and peroxisome proliferator-activated receptor-alpha (PPAR-α) were measured using ELISA kits according to the manufacturers’ instructions, Cat No #MA1-25468 and MBS269041, respectively, purchased from Thermo Fisher Scientific and MyBioSource.
The glucose and lactate metabolism in MCF-7 and MDA-MB-231 cells were measured as described in its corresponding commercial kits, Cat. No# GAGO20 and MAK064 (Sigma-Aldrich) for glucose and lactate, respectively. The glucose and lactate were determined with OD values at 540 nm and 570 nm, respectively, using a spectrophotometer.
Intracellular HK and PDH activities were evaluated with a spectrophotometer using Quantification Kit, Cat. No: MAK091-1KT and MAK183-1KT, respectively, according to the manufacturers’ instructions (Merck KGaA, Darmstadt, Sigma-Aldrich, Germany). The HK and PDH concentrations were determined with OD values at 450 nm.
Western blotting analysis
MCF-7 and MDA-MB-231 cells were seeded at a density of 4 × 105/well in 6-well plates. After treatment, cells were lysed using lysis buffer (10 μl PMSF, 100 mM was added to 1 ml RIPA, Solarbio, Bei**g, China) on ice for 30 min. Cell lysates were separated using 10% SDS-PAGE gels and blotted on polyvinylidene difluoride membranes (PVDFMs), which were blocked with 5% skim milk in PBS containing 0.1% Tween 20 (TBST). Then, the PVDF membrane was incubated overnight with the primary antibodies at 4 °C for 12 h. The following antibodies were used: AKT (in total, 60KDa-Catalog#AHO1112, and phosphorylated form, Ser 473-55.60 KDa-Catalog#44-621G,Thermo fisher), AMPK (in total, 63KDa-Catalog #MA5-14922, and phosphorylated form, Ser485-55KDa-Catalog# PA5-117221,Thermo fisher), PGC-1α (91KDa, Catalog#PA5-72948, Thermo Fisher), TGF-β (44-53KDa, Catalog#MA5-15065, Thermo Fisher), and SIRT-1 (110 KDa, Catalog#PA5-17074, Thermo FISHER) rabbit polyclonal antibodies 1:1000, and the β-actin rabbit polyclonal antibodies 1:4000 (Proteintech, USA) were used as loading controls and for normalization. The secondary antibodies were anti-rabbit antibodies and were conjugated to horseradish peroxidase (1:4000; Proteintech), and were incubated for 1 h at room temperature. The bands were visualized using the ECL reagents (Thermo Fisher Scientific). Band images were obtained by using the Protein Simple Digital imaging system (Flour Chem R, USA).
RNA isolation and real-time PCR analysis
For RNA extraction, the total RNA from MCF-7 and MDA-MB-231 cells was extracted using Trizol Reagent (Thermo Fisher Scientific). cDNA was obtained from total RNA using the PrimeScript™ RT reagent kit (Takara Bio, Inc., Otsu, Japan). The expression of mRNA was assessed by qRT-PCR, which was carried out in triplicate by an SYBR Premix Ex Taq™ kit (Takara Bio, Inc.) and an ABI 7900HT Real-Time PCR system (Thermo Fisher Scientific). The primers used are FR-α (forward primer; CTGGCTGGTGTTGGTAGAACAG and reverse primer; AGGCCCCGAGGACAAGTT) and estrogen-related receptor alpha (ERR-α) (forward primer; GGCCCTTGCCAATTCAGA and reverse primer; GGCCTCGTGCAGAGCTTCT). GAPDH (forward primer; GTCAAGGCTGAGAACGGGAA and reverse primer; AAATGAGCCCCAGCCTTCTC) was used to normalize the results of qRT-PCR and the comparative cycle threshold values (2−ΔΔCt) were adopted to analyze the final results.
Statistical analysis
All experiments were carried out at least in triplicate and the results were expressed as the mean ± standard error of mean (SEM). The statistical analyses were performed using GraphPad Prism software (version 8, La Jolla, CA). Statistical significance between all groups was analyzed by using p < 0.001, p < 0.01 and p < 0.05.
Availability of data and materials
Not applicable.
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This research was funded by the Ministry of Science and Technology, Taiwan (MOST 108-2221-E-006-231-MY3 and 110-2221-E-006-087-MY3).
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Authors and Affiliations
Radiation Biology Department, National Centre for Radiation Research and Technology (NCRRT), Egyptian Atomic Energy Authority (EAEA), Cairo, Egypt
Noura M. Thabet, Mohamed K. Abdel-Rafei & Mostafa A. Askar
Drug Microbiology Lab, Drug Radiation Research Department, National Centre for Radiation Research and Technology, (NCRRT), Egyptian Atomic Energy Authority (EAEA), Cairo, Egypt
Gharieb S. El-Sayyad
Department of Electrical and Electronic Information Engineering, Toyohashi University of Technology, Toyohashi, 441-8580, Japan
Mohamed Abd Elkodous
Department of Radiation Engineering, National Centre for Radiation Research and Technology (NCRRT), Egyptian Atomic Energy Authority (EAEA), Cairo, Egypt
Adel Shaaban
Department of Biomedical Engineering, National Cheng Kung University, Tainan, 70105, Taiwan
Adel Shaaban & Yi-Chun Du
Medical Device Innovation Center, National Cheng Kung University, Tainan, 70105, Taiwan
: Data S1. Stability of DDMPlusAF nanocomposites by DLS and zeta (ζ) potential analyses. Data S2. Cell survival and radio-sensitization of DDM, AF and DDMPlusAF via M-MTT assay at 24, 48 and 72h in comparison: a) MCF-7 and b) MDA cells. Data are mean ± SEM (n = 3), where control cells are set at 100%. Columns with letter a= significant from MCF-7 or MDA cells, b= significant from MCF-7+DDMPlusAF or MDA+DDMPlusAF, c = significant from MCF-7+DDMPlusAF+3Gy or MDA+DDMPlusAF+3Gy, and d = significant from MCF-7+DDMPlusAF+6Gy or MDA+DDMPlusAF+6Gy associated with * = significant from 24 h, # = significant from 48h and @ = significant from72h, in each histogram at P < 0.05. Data S3. Diagram of DDM (a) and AF (b) synthesis.
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Thabet, N.M., Abdel-Rafei, M.K., El-Sayyad, G.S. et al. Multifunctional nanocomposites DDMplusAF inhibit the proliferation and enhance the radiotherapy of breast cancer cells via modulating tumor-promoting factors and metabolic reprogramming.
Cancer Nano13, 16 (2022). https://doi.org/10.1186/s12645-022-00122-1
