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Magnetic resonance hypointensive signal primarily originates from extracellular iron particles in the long-term tracking of mesenchymal stem cells transplanted in the infarcted myocardium

Authors Huang Z, Li C, Yang S, Xu J, Shen Y, Xie X, Dai Y, Lu H, Gong H, Sun A, Qian J, Ge J

Received 21 November 2014

Accepted for publication 28 December 2014

Published 2 March 2015 Volume 2015:10(1) Pages 1679—1690


Checked for plagiarism Yes

Review by Single-blind

Peer reviewer comments 4

Editor who approved publication: Dr Lei Yang

Zheyong Huang,1,* Chenguang Li,1,* Shan Yang,2 Jianfeng Xu,1 Yunli Shen,3 Xinxing Xie,4 Yuxiang Dai,1 Hao Lu,1 Hui Gong,5 Aijun Sun,1 Juying Qian,1 Junbo Ge1

1Shanghai Institute of Cardiovascular Diseases, Zhongshan Hospital, Fudan University, Shanghai, People’s Republic of China; 2Department of Radiology, Zhongshan Hospital, Fudan University, Shanghai, People’s Republic of China; 3Department of Cardiology, Shanghai East Hospital, Tongji University, Shanghai, People’s Republic of China; 4Department of Cardiology, Qianfoshan Hospital, Shandong University, Jinan, Shandong Province, People’s Republic of China; 5Institute of Biomedical Science, Fudan University, Shanghai, People’s Republic of China

*These authors contributed equally to this work

Purpose: The long-lasting hypointensities in cardiac magnetic resonance (CMR) were believed to originate from superparamagnetic iron oxide (SPIO)-engulfed macrophages during long-term stem cell tracking. However, the iron clearance capacity of the ischemic heart was limited. Therefore, we speculated that the extracellular SPIO particles may also be involved in the generation of false-positive signals.
Methods and results: Male swine mesenchymal stem cells (MSCs) were incubated with SPIO for 24 hours, and SPIO labeling had no significant effects on either cell viability or differentiation. In vitro studies showed that magnetic resonance failed to distinguish SPIO from living SPIO-MSCs or dead SPIO-MSCs. Two hours after the establishment of the female swine acute myocardial infarction model, 2×107 male SPIO-labeled MSCs (n=5) or unlabeled MSCs (n=5) were transextracardially injected into the infarcted myocardium at ten distinct sites. In vivo CMR with T2 star weighted imaging-flash-2D sequence revealed a signal void corresponding to the initial SPIO-MSC injection sites. At 6 months after transplantation, CMR identified 32 (64%) of the 50 injection sites, where massive Prussian blue-positive iron deposits were detected by pathological examination. However, iron particles were predominantly distributed in the extracellular space, and a minority was distributed within CD68-positive macrophages and other CD68-negative cells. No sex-determining region Y DNA of donor MSCs was detected.
Conclusion: CMR hypointensive signal is primarily caused by extracellular iron particles in the long-term tracking of transplanted MSCs after myocardial infarction. Consideration should be given to both the false-positive signal and the potential cardiac toxicity of long-standing iron deposits in the heart.

Keywords: superparamagnetic iron oxide nanoparticles, SPIO, cardiac magnetic resonance (CMR), stem cells tracking, extracellular iron particles, myocardial infarction (MI)


Cell transplantation has been considered a promising therapeutic strategy for acute myocardial infarction (MI). However, clinical trials using adult mesenchymal stem cells (MSCs) and other bone marrow-derived cells have indicated that the initial global benefits observed in cardiac function might be slight and transient,1,2 which is partly attributable to the low cell survival and engraftment observed after myocardial delivery.3,4 To address this issue, a non-invasive and in vivo method for tracking cell fate and quantifying cell survival after transplantation needs to be applied.5

Monitoring of stem cells using magnetic resonance imaging (MRI) is based on the imaging of superparamagnetic iron oxide (SPIO) nanoparticles, which causes magnetic field perturbations that can be identified on T2-weighted images.5 Over the past 10 years, many preclinical studies and clinical trials have used SPIO and cardiac magnetic resonance (CMR) imaging to deliver, track, or determine the efficacy of stem cell therapy in the heart.614 The detected signal is used to estimate the number of cells. Even recently, SPIO was still used to label and assess the long-term (2 months) survival of human-induced pluripotent stem cell-derived cardiomyocytes in infarcted myocardia of mini-pigs.15 However, the ability of iron oxide nanoparticles to reliably evaluate long-term stem cell engraftment in the heart has been increasingly suspected. SPIO may not stay inside the transplanted cells over time, but it may be phagocytized by macrophages. Terrovitis et al were the first to report that CMR and ferumoxide cell labeling did not provide reliable information on long-term cell viability and might overestimate ferumoxide-labeled stem cell survival after transplantation.16 Other studies have also reported that long-lasting CMR hypointensities arose from cardiac macrophages that engulfed the SPIO nanoparticles.1719

Conversely, the heart is not a monocyte–macrophage organ, and it has been demonstrated that myocardial iron is cleared more slowly in the heart than in the liver.20 It is difficult for macrophages to move all of the massive SPIO introduced by SPIO-labeled stem cells in the ischemic or necrotic region because of the lack of blood flow and mechanical contraction. Therefore, we speculated the extracellular iron particles may persist in the myocardial interstitial space and may be involved in the generation of hypointensive magnetic resonance (MR) signals in long-term cell tracking.

We conducted this study to explore the composition of the material that produces hypointensities in CMR, and more specifically, to clarify the role of extracellular iron particles in the long-term tracking of SPIO-labeled MSCs in a swine model of MI.

Materials and methods

Cell preparation and labeling

MSCs were isolated from male swine (from the Shanghai Animal Administration Center) and cultured at 37°C in a 5% CO2 incubator, as previously described.21,22 Dulbecco’s Modified Eagle’s Medium (DMEM) (Thermo Fisher Scientific, Waltham, MA, USA) with 10% fetal bovine serum (FBS) (Thermo Fisher Scientific) and penicillin-streptomycin (Thermo Fisher Scientific) was used as a standard culture medium. All cells used in this study were of second to third passage with a confluency of 80%–90%.

To label the MSCs, we used an injectable solution of ferumoxides, a type of SPIO (50 μg Fe/mL Resovist; Schering AG, Berlin, Germany) combined with poly-L-lysine (average molecular weight [MW] 275 kDa) (Thermo Fisher Scientific). Resovist was added to the serum-free culture medium (final concentration: Resovist 50 μg/mL, poly-L-lysine, 1.5 μg/mL) and mixed for 60 minutes with intermittent shaking by hand; the MSCs were then incubated with this mixture for 24 hours, as described previously.23 Before injection, the medium was discarded, and the cells were washed twice with phosphate-buffered saline (PBS), treated with trypsin (Thermo Fisher Scientific), collected, rewashed, and counted to adjust the cell concentration for the transplantation.

To evaluate the labeling efficacy, Prussian blue staining (potassium ferrocyanide and HCl solution from Juesheng Biotechnology Co, Ltd, Shanghai, People’s Republic of China) and electron microscopy (Philips CM120; Philips NV, Amsterdam, the Netherlands) were undertaken to indicate the presence and localization of intracellular iron particles. To determine the attenuation of iron content in cells over time, labeled MSCs continued to be cultured in medium, and the iron content of the cells was quantified every 4 days using atomic absorption spectrometry (Thermo E.IRIS Duo ICP; Thermo Fisher Scientific).

Cellular proliferation, viability, and differentiation

The proliferation and viability of unlabeled MSCs and SPIO-labeled MSCs were compared. In the proliferation assays, cells were seeded at 3×105 cells/flask, and the medium was changed every 3 days. At subconfluence (90%), the cells were detached with Accutase (GE Healthcare Europe GmbH, Freiburg, Germany) and counted with a CASY®2 Analyzer (CASY®2-Cell Counter and Analyzer System, Model TT; Hoffman-La Roche Ltd, Basel, Switzerland). The experiments were performed in triplicate. Cellular viability under the various conditions was examined according to both the Electrical Current Exclusion (ECE) method described by Lindl et al24 and the viability standard operational procedure of the manufacturer.

To evaluate the adipogenic differentiation potential, MSCs and SPIOs-MSCs were cultured in Adipogenic inductive medium (SR811D250; Amsbio, Madrid, Spain) for 21 days (medium was changed every 3 or 4 days).25 Untreated cells were maintained in DMEM with 10% FBS. Oil droplets in differentiated adipocytes were evaluated by Oil red O staining (Sigma-Aldrich Co, St Louis, MO, USA) after 21 days.

To determine the differentiation of myocardium-like cells, MSCs and SPIO-MSCs were cultured in culture medium with added 5-aza-2′-deoxycytidine (5-aza-C; Sigma-Aldrich Co) for 24 hours. Incubation then continued in complete medium lacking 5-aza-C, with medium changes every 3 days. Undifferentiated MSCs and normal mature swine cardiomyocytes were used as negative and positive controls, respectively. Total RNA was extracted from cultured cells using TRIzol reagent (Thermo Fisher Scientific) according to the manufacturer’s protocol. Reverse transcriptase polymerase chain reaction (RT-PCR) primers (synthesized by Shanghai Sangon Biological Engineering Technology and Service Co, Shanghai, People’s Republic of China) were as follows:25 cTnT, 5′-CCA GAA GAC AGA GCG GAA AA-3′ and 5′-CGG GTC TTG GAG ACT TTC TG-3′; Desmin, 5′-ATG TCC AAG CCA GAC CTC AC-3′ and 5′-GCC TCA TCA GGG AAT CGT TA-3′; α-cardiac actin, 5′-ATG GTG GGT ATG GGT CAG AA-3′ and 5′-TAC ATG GCA GGG ACA TTG AA-3′; and glyceraldehyde 3-phosphate dehydrogenase (GAPDH), 5′-GGG CAT GAA CCA TGA GAA GT-3′ and 5′-AAG CAG GGA TGA TGT TCT GG-3′. Transcriptional expressions of cTnT, Desmin, and α-cardiac actin genes from the MSCs and SPIO-MSCs were determined by RT-PCR according to the manufacturer’s instructions. Transcription levels were standardized to the corresponding swine GAPDH level.

In vitro MR imaging of SPIO and MSCs

To evaluate the in vitro MR imaging of SPIO and MSCs under different conditions, 5×105 unlabeled MSCs, 5×105 living SPIO-MSCs, 5×105 dead SPIO-MSCs (treated with 75% alcohol solution for 10 minutes, and confirmed by trypan blue exclusion test), and SPIO alone (iron content equivalent to 5×105 SPIO-labeled MSCs) were resuspended in 0.5 mL 0.3% agarose gel in an Eppendorf (EP) tube. MR imaging was performed using a 1.5-T MR scanner (CV/i; GE Healthcare Europe GmbH) with a 90 cm field of view (FOV), three acquisitions, 4 mm slice thickness with no gap, and a 512×512 matrix. Imaging sequences were as follows: 1) spin echo (SE) sequence: T1 weighted imaging (T1WI), repetition time (TR) =450 ms, echo delay time (TE) =9 ms; 2) fast spin echo (FSE) sequence: T2 weighted imaging (T2WI), TR =4,800 ms, TE =96 ms; and 3) T2 star weighted imaging (T2*WI) flash sequence: T2*WI, TR =800 ms, TE =26 ms.

The signal intensity in each EP tube was obtained. The change of signal intensity relative to the unlabeled MSCs was calculated as the following:


All experiments were performed in triplicate for each set of conditions.

Swine MI model

Animal experiments were approved by the Animal Care and Use Committee of Fudan University, Shanghai, People’s Republic of China and were in compliance with the Guide for the Care and Use of Laboratory Animals published by the National Research Council (US) Institute for Laboratory Animal Research.26 Twenty-two female miniature swine (8–11 months old, weighing 18.9–25.1 kg) were obtained from the Shanghai Animal Administration Center, Shanghai, People’s Republic of China. The swine fasted for 6 hours and were sedated with ketamine (15–20 mg/kg), diazepam (1.5–2 mg/kg), and atropine (50–100 μg/kg). The anesthesia was maintained with pentobarbital sodium (0.1–0.2 mg/kg/min, intravenously), during which succinylcholine (10 mg/kg) was added to ensure thorough muscular relaxation when necessary. All animals were intubated and mechanically ventilated. Subsequently, the heart was exposed through a lateral thoracotomy. Anterior MI was created by ligation of the left anterior descending artery (LAD) at two-thirds of the distance from the apex.27 The electrocardiogram (ECG) was recorded to confirm the presence of infarction. A lidocaine bolus (2 mg/kg) was given before coronary occlusion. Following occlusion, lidocaine was infused intravenously at a rate of 50 μg·kg−1·min−1.

Cardiac MR imaging and tracking of SPIO-MSCs in vivo

To verify the in vivo MR imaging of SPIO and MSCs under different conditions, 2 hours after the ligation of LAD, unlabeled MSCs (1×106/150 μL), living SPIO-labeled MSCs (1×106/150 μL), dead SPIO-labeled MSCs (1×106/150 μL, and SPIO (150 μL, iron content equivalent to 1×106 SPIO-labeled MSCs) were injected into the peri-infarct areas with a 27-gauge needle (Thomas Scientific, Swedesboro, NJ, USA) (n=3 in each group). Then, the animals were transferred for CMR imaging without following up.

To explore the value of SPIO in the long-term CMR tracking of transplanted cells, 2×107 SPIO-labeled MSCs were injected at ten injection sites (each injection =2×106/150 μL) into the peri-infarct areas with a 27-gauge needle (swine, n=5) 2 hours after the ligation of LAD. A further MI swine with DMEM injection served as medium controls (swine, n=5). CMR was performed at 3 days, and 1, 3, and 6 months after infarction.

To visualize SPIO-labeled MSCs, high-resolution CMR images were obtained using a 1.5-T MR scanner (CV/I; GE Healthcare Europe GmbH), as previously described.28 Twelve to 18 contiguous short-axis images were acquired, covering the entire left ventricle, by applying ECG-triggered T2WI-flash sequence. The imaging parameters were as follows: TR =122 ms; TE =12.1 ms, flip angle =25°; 512×512 matrix; 4 mm slice thickness with no gap; 32 kHz bandwidth; 28 cm FOV; and three acquisitions (number of signal averaged, NSA).

Histopathological analysis

Animals were sacrificed at the end of the observation period. To identify the origin of hypointensities in CMR, a series of consecutive sections was examined by combining hematoxylin eosin (HE) staining, Prussian blue staining, and anti-human macrophage (CD68) immunohistochemical staining. For Prussian blue staining, which indicates the presence of iron, the tissue sections were incubated for 30 minutes with 2% potassium ferrocyanide (ie, Perl reagent) in 6% HCl and counterstained with nuclear fast red. The sections were examined using standard immunohistochemical techniques with CD68 monoclonal antibody (Clone No PM-1K Gentaur, and a DAB kit (Juesheng Biotechnology Co, Ltd). CD68 positive cells appeared with brown staining.


To identify the survival of transplanted male MSCs 6 months after cell transplantation, RT-PCR analysis for the swine SRY gene was conducted on DNA from infarcted hearts of female recipients treated with either MSCs from donor males or media. Genomic DNA was isolated using a Genomic DNA Isolation Kit (Qiagen NV, Venlo, the Netherlands). RT-PCR was conducted, as described previously29 using an ABI Prism 7700 sequence detection system (Thermo Fisher Scientific). Standard curves were generated by serially diluting male swine genomic DNA prepared from male MSCs. The sequence of the PCR primers used for detection of swine male-specific SRY gene was as follows: 5′-AAA GCG GAC GAT TAC AGC-3′ and 5′-TTT GCA TTT GAG GGT TCT-3′. RT-PCR protocol consisted of an initial step at 94°C for 2 minutes, followed by 38 cycles of the following: denaturation at 94°C for 30 seconds, annealing at 50°C for 30 seconds, and elongation at 72°C for 30 seconds.

Statistical analysis

Descriptive variables were presented as the mean ± standard deviation (SD). Comparisons between two groups were conducted using the unpaired Student’s t-test. Comparisons among more than two groups were determined by a one-way analysis of variance (ANOVA) test and Bonferroni post hoc test. All statistical analyses were performed using the SPSS system (SPSS for Windows 15.0; SPSS Inc, Chicago, IL, USA). Values of P<0.05 were considered statistically significant.


Iron labeling and release rate

SPIO-labeled MSCs showed abundant intracytoplasmic blue inclusions following Prussian blue staining, and the labeling efficiency was nearly 100%. Although the cells had been washed by PBS several times before Prussian blue staining, a small amount of extracellular blue particles remained attached to the surface of cells. Transmission electron microscopy of labeled cells indicated the presence of the anionic magnetic nanoparticles exclusively in polydisperse vesicles in the cytoplasm (Figure 1).

Figure 1 Cell labeling.
Notes: (A) Non-labeled bone marrow-derived mesenchymal stem cells in vitro (×100). (B) Prussian blue-stained, labeled cells (×100). The majority of blue-stained iron particles were distributed in the cytoplasm, whereas a small amount of particles adhered to the cell membrane (red arrows in inset). (C) Electron microscopic images of labeled MSCs shows dense particles (red arrows) clustered within the cytoplasm.

The intracellular mean iron load (23.77±6.06 pg/cell) at day 0 decreased with the duration of culturing after magnetic labeling and was comparable with that of the non-labeled MSCs at day 20 (Figure 2A, B) (0.29±0.10 pg/cell vs 0.21±0.06 pg/cell; P>0.05), indicating the fast rate of the physiological release process of intracellular iron particles. Such a release process of iron could be occasionally observed by electron microscopy (Figure 2C).

Figure 2 Release rate of intracellular iron in vitro.
Notes: (A) Prussian blue staining of SPIO-MSCs at different times after SPIO labeling (all figures in A are at 50 μm in size range). (B) Quantitative analysis showing that the intracellular mean iron load decreased continuously over time after magnetic labeling. (C) Electron microscopic images of MSCs at 4 days after labeling showed the release of iron dense particles (red arrow) from the cytoplasm.
Abbreviations: d, days; SPIO, superparamagnetic iron oxide; MSCs, mesenchymal stem cells; SPIO-MSCs, mesenchymal stem cells incubated with superparamagnetic iron oxide.

The effects of SPIO labeling on cellular proliferation, viability, and differentiation

The proliferation rate and viability showed no differences between unlabeled and SPIO-labeled MSCs (Figure 3AB). To determine the adipogenic differentiation, the MSCs and SPIO-MSCs were cultured for 21 days in adipogenic media. As shown in Figure 3C, both MSCs and SPIO-MSCs differentiated into the adipogenic lineages, as evidenced by multivacuolar cells, with the secretion of neutral lipid droplets and confirmed by Oil red O staining. Following myocardial differentiation, RT-PCR showed that myocardial genes cTnT, Desmin, and α-cardiac actin were all detected in both differentiated MSCs and SPIO-MSCs (Figure 3D). The expression of these myocardial genes was comparable between differentiated MSCs and differentiated SPIO-MSCs (Figure 3E). These results suggest that a low concentration of SPIO labeling did not affect the proliferation, viability, and differentiation capacity of MSCs.

Figure 3 Proliferation, viability, and differentiation capacity of SPIO-MSCs.
Notes: (A) Proliferation rate of SPIO-MSCs. (B) Viability rate of SPIO-MSCs. (C) Oil red O staining for adipogenic differentiation (both images in C are at 100 μm in size range). (D) RT-PCR for myocardial gene cTnT, desmin, and α-cardiac actin. (E) Quantitative gene expression analysis. SPIO labeling did not affect the proliferation, viability, and differentiation capacity of MSCs.
Abbreviations: MSCs, mesenchymal stem cells; SPIO, superparamagnetic iron oxide; SPIO-MSCs, mesenchymal stem cells incubated with superparamagnetic iron oxide; RT-PCR, real-time quantitative polymerase chain reaction; GAPDH, glyceraldehyde 3-phosphate dehydrogenase; NS, not significant; NC, negative control; PC, positive control.

In vitro MR imaging of SPIO and MSCs

Compared with unlabeled MSCs (5×105), living SPIO-MSCs (5×105), dead SPIO-MSCs (5×105) and SPIO alone (0.6 μL Resovist) showed similar changes in their MR signals: SE T1WI signal increased slightly, while FSE T2WI and T2*WI-flash signal reduced obviously (Figure 4A). The change of signal intensity relative to the unlabeled MSCs (SI) showed no significant difference among the living SPIO-MSCs, the dead SPIO-MSCs, and the SPIO-alone groups (Figure 4B; all groups P>0.05), suggesting that the magnetic signal originates from SPIO itself, regardless of its location (within or outside of cells) and cell survival status (living or dead).

Figure 4 In vivo magnetic resonance imaging.
Notes: (A) In vivo magnetic resonance imaging of tube-containing gel with 5×105 unlabeled MSCs, living SPIO-MSCs, dead SPIO-MSCs, and SPIO alone (0.6 μL Resovist) without MSCs, respectively. (B) Quantitative analysis of signal intensity. Equation for SI is SI = [(SI−SIunlabeled MSCs)/SIunlabeled MSCs] ×100%.
Abbreviations: MSCs, mesenchymal stem cells; SPIO, superparamagnetic iron oxide; SPIO-MSCs, mesenchymal stem cells incubated with superparamagnetic iron oxide; SI, signal intensity; FSE, fast spin echo; T1WI, T1 weighted imaging; T2WI, T2 weighted imaging; T2*WI, T2 star weighted imaging.

In vivo CMR imaging of SPIO and MSCs

In the three SPIO-containing groups (ie, the living SPIO-MSCs group, the dead SPIO-MSCs group, and the SPIO alone group), CMR imaging with a T2WI-flash sequence showed the same signal void (dark region) corresponding to the initial injection sites in the myocardium. However, signal-void lesions were not detected at the injection sites in the unlabeled MSC group (Figure 5). This result was consistent with in vitro cellular MR imaging, confirming that the magnetic imaging cannot distinguish between intracellular iron and extracellular iron, let alone between living cells and dead cells.

Figure 5 CMR imaging.
Notes: (A) Representative in vivo CMR imaging of injected 5×105 unlabeled MSCs, (B) living SPIO-MSCs, (C) dead SPIO-MSCs, and (D) SPIO (0.6 μL Resovist) in swine heart. Red arrows in figures BD indicate the signal void corresponding to the injection sites. (E) Quantitative analysis of signal intensity. SI=[(SI-SIunlabeled MSCs)/SIunlabeled MSCs]×100%.
Abbreviations: CMR, cardiac magnetic resonance; LV, left ventricle; MSCs, mesenchymal stem cells; NS, not significant; RV, right ventricle; SPIO, superparamagnetic iron oxide; SPIO-MSCs, mesenchymal stem cells incubated with superparamagnetic iron oxide; SI, signal intensity.

Long-term signal tracking by CMR

For the long-term CMR tracking of transplanted cells, CMR with T2WI-flash sequence was performed at 3 days, and 1, 3, and 6 months after MSC injection in the peri-infarct areas. The SPIO-labeled MSCs were identified as a signal void corresponding to the initial injection sites, whereas no signal-void lesion was detected in the medium control group. In the SPIO-labeled MSCs group, 6-month serial MR images revealed that the signal-void areas gradually became less contrasted and more blurred over time (Figure 6A). However, the majority of signal-void areas could persist for a long time, as evidenced by 39 (78%), 37 (74%), 36 (72%), and 32 (64%) of the 50 sites being identified at 3 days, and 1, 3, and 6 months after transplantation, respectively (Figure 6B).

Figure 6 Long-term CMR tracking.
Notes: (A) Representative serial long-axis views imaged at 3 d, 1 m, 3 m, and 6 m after infarction show the signal void (red arrows) gradually faded over time. (B) The number of visible injection sites by CMR gradually decreased over time post-injection.
Abbreviations: CMR, cardiac magnetic resonance; d, days; m, months.

Histological analysis

Histology of swine hearts was performed at 6 months after cell injection. In contrast to the persistence of hypointensive areas in CMR, no SRY sequences were detected in any of the female recipients treated with labeled MSCs, indicating that no donor MSCs survived at 6 months after cell transplantation.

On histology, massive iron (Prussian blue-positive) deposits were detected at the injection sites in tissue sections corresponding to the hypointensive signal areas in CMR. Interestingly, the deposits were almost all located in fibrous tissue, and no Prussian blue-positive deposit was observed in the normal myocardium in the peri-infarct region. The iron particles could be categorized into three groups based on the consecutive staining by HE, Prussian blue, and CD68 (a macrophage-specific antigen). First, the majority of iron particles were distributed extracellularly (red arrowhead, Figure 7AC). Second, a certain number of CD68-positive macrophages or giant multinucleated cells were co-localized with the marginal zone of a massive iron area (Figure 7C1), indicating that macrophages engulfed a portion of the iron particles. Third, a small amount of iron particles was dispersed in the surrounding areas of massive iron accumulation. In a magnified view, some of them were distributed evenly around the nucleus, forming a spherical shell-like pattern23 and indicating an intracellular location (Figure 7B2). However, such interstitial cells that internalized iron were negative for CD68 staining.

Figure 7 Representative histology of the injection sites 6 months after cell injection.
Notes: (A) HE staining. A1 is the inset of A and shows the giant multinucleated cells. (B) Prussian blue staining. B1 inset shows the giant multinucleated cells at the corresponding site to A1 inset. (B2) inset shows the iron-containing, small-sized, non-macrophage interstitial cells. (C) CD68 immunohistochemical staining. C1 inset showing the CD68-positive giant multinucleated cells at the corresponding site to A1 inset and B1 inset. Massive Prussian blue-positive iron deposits were detected at the injection sites. Iron particles were predominantly distributed in the extracellular space (red arrows in AC), whereas a minority of iron particles were distributed within CD68-positive macrophages (white arrows in A1, BI and C1) and other CD68-negative cells (black arrows in B2).
Abbreviation: HE, hematoxylin eosin.

These findings indicated that the long-lasting CMR signal primarily originated from extracellular iron particles and was only partly attributable to the intracellular iron particles. There was no relation of transplanted MSCs to the persistence of CMR hypointensities.


Before this work, the prevalent view was that CMR of SPIO-labeled stem cells did not provide reliable information on long-term cell viability and might overestimate stem cell survival after transplantation; further, the long-lasting CMR hypointensities were believed to arise from the cardiac macrophages that engulfed the SPIO nanoparticles.1619 Here, we found that the long-lasting CMR signal in the long-term tracking of transplanted stem cells after MI originated primarily from extracellular iron particles, rather than from intracellular iron particles.

The persistence of SPIO particles in the infarcted myocardium may be attributed to the imbalance between the massive iron release from the transplanted cells and the relatively limited iron removal capacity of the heart. Figure 8 illustrates the source and clearance of the extracellular SPIO particles. The main source of the SPIO is dead labeled cells. Due to the harsh environments, the fraction of transplanted cells that survive to later time points is typically less than 1%30 and may even be undetectable, as shown in this study. Even in the living stem cells, the attenuation of intracellular iron is quite rapid, as demonstrated in our in vitro study. A small amount of the SPIO attached to the surface of transplanted cells could also directly deposit in the myocardium. Additionally, MI or therapeutic intramyocardial injection may result in an iron-containing hemorrhage. The SPIO particles could be removed from the myocardium through a two-step process: first, by being engulfed by endogenous host cells such as macrophages, and then by being taken away by muscle contraction and coronary flow. However, the heart is quite different from the liver, spleen, and other monocyte–macrophage organs, which are rich in monocyte-like or macrophage-like cells. Although circular monocyte–macrophage will be attracted to and supply the scarce resident macrophages, the injected SPIO is very easily accumulated in situ16,20 because of the lack of blood flow and mechanical contraction in the ischemic or necrotic region. It is logical to assume that once the amount of SPIO or iron particles goes beyond the phagocytic capability of macrophages, the remaining SPIO will subsequently deposit in the interstitial tissue of the heart.

Figure 8 The source and clearance of the extracellular SPIO particles in the myocardium.
Abbreviations: MSC, mesenchymal stem cell; SPIO, superparamagnetic iron oxide.

A possible explanation for the discrepancy in iron location between our study (extracellular) and other studies showing an intracellular location1619 is the differences observed in the properties of the SPIO particles. It has been reported that SPIO with different sizes, coatings, and composition showed a high variation in their potential to be phagocytized by monocyte–macrophages and non-phagocytic cells.3133 A second hypothesis is that the follow-up period in the present study was longer than those in others and that more SPIO-phagocytized cells will die in an adverse environment with more fibrotic tissues. However, the specific mechanism and process involving the iron clearance needs to be studied further, and the effect of desferrioxamine treatment in removing myocardial iron also merits further investigation.

The iron particles introduced by SPIO-MSCs were not able to be removed effectively by the heart, which may have a negative impact on long-term cell tracking. This study showed that the magnetic void signal originated primarily from iron itself, regardless of its location (within or outside of cells) and cell survival status (living or dead). Consistent with other studies,1619 the present study confirmed that CMR of SPIO-labeled MSCs was not a reliable technique to track and quantify cells that are injected in vivo into the heart. For long-term tracking, therefore, one must be cognizant that hypointensities may overestimate the number of viable cells if free SPIO or phagocytic cells persist in the tissue.17

It is worth noting that long-standing SPIO deposition may have the potential to injure cardiac cells. Although our in vitro study showed that a low concentration of SPIO had no significant effects on MSCs’ viability and differentiation, concerns should be noted about its potential cardiac toxicity for the following reasons. First, despite being coated with a polymer structure, SPIO can still be biodegraded into free iron if in the body for a long time. High levels of free ferrous iron can react with peroxides to produce free radicals, which are highly reactive and can damage cellular components. Therefore, SPIO has the potential to cause oxidative stress.3436

Second, the heart is considered one of the most sensitive organs to iron overload.20 It is well known that iron overload could cause cardiomyopathy with clinical manifestations, including decreasing the cardiac ejection fraction and arrhythmia.3739 Acidic environments prompt the transformation of iron from the oxidation state (Fe3+) to the reduced state (Fe2+), resulting in the generation of oxygen free radicals. Therefore, the toxic effect of myocardial iron is dynamic and is increased in the presence of metabolic acidosis.40 Based on the available data, it is logical to assume that peri-infarct ischemic myocardium, the target for SPIO-mediated stem cell therapy, is particularly susceptible to iron toxicity.

Third, when intramyocardially injected with SPIO-labeled stem cells, the local myocardium will deposit massive amounts of SPIO for a very long time, as shown in our study. The quantity and duration of SPIO deposition in the myocardium is far beyond that observed in previous intravenous studies,4143 in which SPIO was administered systemically and proved to be a safe and efficient MR contrast agent. The situation is even worse in the context of SPIO-based magnetic targeting therapy, which was recently introduced for treating cardiovascular diseases,4447 in which more SPIO, alongside therapeutic drugs/cells, will be homing to the target area of the heart.

Fourth, as shown in this study, the iron particles were almost all located in fibrous tissue, and no iron deposits were observed in the normal myocardium in the peri-infarct region at 6 months after cell injection. This difference may be related to the normal removal capacity of the normal myocardium; however, it cannot be excluded that myocardial fibrosis was induced by iron toxicity. Therefore, the safety of SPIO-based cell therapy, especially the safety issues surrounding the influence of local SPIO particles on myocardial function, requires further investigation. Future research methodologies based on fuzzy clustering and fuzzy regression methods may also be helpful.48

Another interesting finding of this study is the presence of iron-containing, small-sized, non-macrophage cells in the myocardial interstitial tissue. Intracytoplasmic iron inclusions were distributed evenly around the nucleus of cells as a spherical shell (Figure 7B2). In view of the negative CD68 staining and no SRY gene detected, these cells seem unlikely to be MSC-differentiated cells or macrophages. Further studies are required to identify the specific cell type and its exact role in iron removal.


Ultimately, this study demonstrated that SPIO is of limited value in the long-term MR tracking of transplanted cells after MI and that the MR hypointensities primarily originate from extracellular iron particles. The potential toxicity of long-standing iron deposition in the heart should be considered.


The authors gratefully acknowledge financial support from the National Natural Science Foundation of China (grants 81370003, 81470467, 81000043, 81300095, and 81400318), the Natural Science Foundation of Shanghai Municipality of China (grant 15ZR1434100), and the Science and Technology Commission of Shanghai Municipality (grant 13JC1401703).


The authors declare no conflicts of interest in this work.



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