- Open Access
Changes in intrathoracic pressure, not arterial pulsations, exert the greatest effect on tracer influx in the spinal cord
Fluids and Barriers of the CNS volume 19, Article number: 14 (2022)
Cerebrospinal fluid (CSF) circulation in the brain has garnered considerable attention in recent times. In contrast, there have been fewer studies focused on the spine, despite the expected importance of CSF circulation in disorders specific to the spine, including syringomyelia. The driving forces that regulate spinal CSF flow are not well defined and are likely to be different to the brain given the anatomical differences and proximity to the heart and lungs. The aims of this study were to determine the effects of heart rate, blood pressure and respiration on the distribution of CSF tracers in the spinal subarachnoid space, as well as into the spinal cord interstitium.
In Sprague Dawley rats, physiological parameters were manipulated such that the effects of spontaneous breathing (generating alternating positive and negative intrathoracic pressures), mechanical ventilation (positive intrathoracic pressure only), tachy/bradycardia, as well as hyper/hypotension were separately studied. To investigate spinal CSF hydrodynamics, in vivo near-infrared imaging of intracisternally infused indocyanine green was performed. CSF tracer transport was further characterised with in vivo two-photon intravital imaging. Tracer influx at a microscopic level was quantitatively characterised by ex vivo epifluorescence imaging of fluorescent ovalbumin.
Compared to mechanically ventilated controls, spontaneous breathing animals had significantly greater movement of tracer in the subarachnoid space. There was also greater influx into the spinal cord interstitium. Hypertension and tachycardia had no significant effect on spinal subarachnoid spinal CSF tracer flux and exerted less effect than respiration on tracer influx into the spinal cord.
Intrathoracic pressure changes that occur over the respiratory cycle, particularly decreased intrathoracic pressures generated during inspiration, have a profound effect on tracer movement after injection into spinal CSF and increase cord parenchymal tracer influx. Arterial pulsations likely drive fluid transport from perivascular spaces into the surrounding interstitium, but their overall impact is less than that of the respiratory cycle on net tracer influx.
The interaction between CSF and interstitial fluid (ISF) is vital for many homeostatic functions in the central nervous system (CNS) [1,2,3]. Many investigators have proposed that the interface between the two fluids occurs at spaces around penetrating blood vessels—the perivascular spaces—with additional interactions via transpial and transependymal routes [3,4,5]. The precise anatomical configuration of the perivascular space, as well as the mechanisms that mediate fluid and solute exchange, have not been fully elucidated . In the brain, there are compelling data, largely derived from human magnetic resonance imaging (MRI) and computational modelling studies, that physiological forces such as arterial pulsations and respiratory pressures drive fluid flow in the subarachnoid space [7,8,9,10]. Negative intrathoracic pressures generated during the inspiratory period of the respiratory cycle produce high CSF flow, overshadowing the cardiac component [11,12,13,14]. MRI studies have been critical for recent advances in imaging CSF flow, however, they are limited by their spatial resolution, preventing the study of fluid and solute exchange between CSF and CNS tissue. Currently, only invasive animal experiments can garner this information.
An in vivo two-photon excitation imaging study investigating CSF flow in mouse brain suggested that increasing blood pressure reduced the overall flow in perivascular spaces around arterioles . However, the relative influence of respiration vs arterial pulsations has not been studied in animals. In addition, the dynamics that mediate flow in the spinal cord cannot simply be extrapolated from intracranial studies. Previous work in rat spinal cord by our group, albeit using ex vivo studies, has demonstrated shared pathways for CSF tracer transport around peri-arterial and peri-venous spaces , which is in contrast to the glymphatic theory reported in some studies of the mouse brain [17,18,19]. Not only is the spinal cord parenchyma anatomically different compared to the brain (the grey and white matter are reversed), but the extradural venous anatomy is configured such that there is direct exposure of the epidural venous plexus to intrathoracic pressures . There have been no previous attempts to independently examine the effects of blood pressure, heart rate and negative intrathoracic pressures generated during inspiration on spinal cord fluid dynamics.
To comprehensively assess the impact of cardiorespiratory drivers on spinal CSF flow and CSF/ISF exchange, fluorescent tracers were injected into the cisterna magna of Sprague Dawley rats. To evaluate cervicothoracic spinal CSF bulk flow, a novel in vivo, near infrared (NIR) imaging technique using indocyanine green (ICG) as a CSF tracer was employed. Two-photon excitation imaging was utilized to characterize the movement of individual molecules (1.0 µm FluoSpheres™) in vivo at the microscopic level. Finally, we performed ex vivo analysis of tracer redistribution microscopically in the spinal interstitium (through axial sections of the spinal cord). The effects of hypertension (pharmacologically induced), heart rate (induced by sinoatrial node pacing) and negative intrathoracic pressure in spontaneously breathing rats were compared to control animals maintained using positive pressure ventilation. Transport of fluorescent tracers in the spinal cord were investigated after manipulation of each of the three physiological variables. It was hypothesised that negative intrathoracic pressures would result in greater molecular transport/CSF flow, while elevated pulse pressure and tachycardia would reduce net movement.
Materials and methods
Male Sprague Dawley rats (aged between 8 and 12 weeks and weighing 280–430 g) were used in all experiments. Ethics approval was obtained from the Animal Ethics Committees of Macquarie University (Protocol No. 2016/032) and the University of Sydney (Protocol No. 2018/1402).
After induction of general anaesthesia with 5% isoflurane in oxygen, each animal was positioned supine on a heating pad and maintained under anaesthesia with isoflurane in 0.2 L/min of oxygen. Heart rate, oxygen saturation, respiratory rate, and temperature were continuously monitored by pulse oximetry and rectal thermometer. Rats undergoing two-photon excitation microscopy were pre-medicated with subcutaneous midazolam (1 mg/kg) and buprenorphine (0.05 mg/kg) prior to anaesthesia with isoflurane.
A right transverse inguinal incision was made, and the femoral neurovascular bundle was exposed for cannulation by arterial and central venous polyethylene catheters. This was followed by a midline suprasternal incision. The trachea was exposed for insertion of an endotracheal tube. This was connected to a respiratory circuit, delivering isoflurane in oxygen. The egress tubing was connected in series to a capnometer (Capstar-100, CWE Inc., Ardmore, PA, USA), for continuous end-tidal carbon dioxide (CO2) monitoring, as well as to a custom-made respiratory circuit pressure manometer. At this point, for the subset of rats where heart rate was modulated, a 3-cm length of the right external jugular vein was dissected out. A custom manufactured atrial pacing wire was inserted into this vein to rest just above the sinoatrial node. The pacing wire was connected to an isolated pulse stimulator (A-M Systems Inc, model 2100) .
The animal was then repositioned prone and the respiratory circuit manometer and arterial line were connected to pressure transducers, enabling the continuous measurement of blood pressure and circuit pressure. All vital statistics were recorded continuously for the remainder of the experiment on a data acquisition interface, Power1401 (Cambridge Electronic Device, Cambridge, UK). Arterial blood gas was analysed for pH, partial pressure of oxygen, and partial pressure of CO2. Each physiological variable—respiration, blood pressure and heart rate—was then manipulated in isolation to investigate its effect on spinal subarachnoid space flow and parenchymal inflow (Fig. 1).
Modulation of physiological parameters
To examine the effects of negative intrathoracic pressure generated by spontaneous respiration, rats were either allowed to breathe spontaneously on the respiratory circuit, or a neuromuscular blockade was administered (pancuronium bromide 0.8 mg induction, 0.4 mg/h maintenance) followed by mechanical ventilation using a small animal ventilator (Harvard 7025 Rodent Ventilator, set at a tidal volume of approximately 1.2 mL). Any prolonged vagolytic effects of pancuronium resulting in hypertension and tachycardia were reversed with small boluses of metoprolol (15 mg/kg). The end tidal CO2 was adjusted to a physiological range of 3.5–4.5%. In anaesthetised spontaneously breathing rats, bradypnoea of 50–55 breaths/min was observed, with resultant CO2 retention and respiratory acidosis. Therefore, control animals underwent positive pressure ventilation with a respiratory rate and blood gas profile matching that of their spontaneous breathing counterparts. Since these animals were under isoflurane anaesthesia they had low heart rates and blood pressures. This control group was also used for the blood pressure and heart rate experiments. Other variables including mass, heart rate, and mean arterial pressure (MAP) were kept constant between spontaneous breathing and control groups.
To examine the effects of blood pressure, hypertensive rats were compared to the mechanically ventilated group(s), which had an approximate MAP of 70 mmHg. In hypertensive rats, the MAP was raised to a target of 140 mmHg (a ~ 40% increase from the normal base value, or approximately double that of controls) by an escalating infusion of phenylephrine (20–200 µg/kg/min), a selective α1-adrenergic receptor agonist. In order to maintain a constant heart rate and prevent baroreflex compensation, the nicotinic receptor antagonist hexamethonium (20–25 mg/kg) was administered. All hypertensive animals were mechanically ventilated to relative hypercapnic levels (matching the Control group). Mass, heart rate, and ventilation were kept constant between hypertensive and control groups.
To examine the effect of heart rate, tachycardic rats were compared to the mechanically ventilated group(s), which had an approximate heart rate of 330 beats/min (bpm). A pacing wire (described above) was connected to an isolated pulse generator (A-M Systems Inc, model 2100). A square pulse duration of 2 ms and an amplitude aiming for 1.0 V was used to generate a heart rate of at least 500 bpm. There was no appreciable change in blood pressure on pacing, even over prolonged periods. All tachycardic animals were mechanically ventilated to a relative hypercapnic level (matching the Control group). Mass, MAP, and ventilation were kept constant between tachycardic and control groups.
Ventilation rate/blood gas profile
To determine if blood pH, partial pressure of CO2, and rate of ventilation have an effect on ISF/CSF fluid dynamics, an additional control group (Normal), maintained with positive pressure ventilation to a higher respiratory rate of 66 breaths/min, which normalised partial pressure of CO2 and pH, was introduced. Since the likely consequence of acidosis is dilatation of penetrating arterioles , it was hypothesised that the greatest effect of altering respiratory rate would be observed on tracer influx into the spinal cord parenchyma. Thus, a higher respiratory rate control group with normal physiology was introduced in the ex vivo studies investigating the effect of respiration, blood pressure, and heart rate on the distribution of tracer.
Surgical procedures for investigation of fluid dynamics
After the desired physiological parameter target was reached and maintained, one of three surgical procedures was performed to investigate fluid transport in the spinal subarachnoid space, and into the spinal cord. CSF tracer movement was assessed using one of the following fluorescent tracers injected into the cisterna magna: ICG (Verdye, Aschheim-Dornach, Germany); 1 μm FluoSpheres™ (13% v/v: ThermoFisher Scientific, Massachusetts, USA), Ovalbumin Alexa-Fluor®-647 conjugate (AFO-647: Life Technologies, Victoria, Australia). CSF tracer movement was imaged using NIR intravital imaging, two-photon microscopy, and ex vivo microscopy.
NIR intravital imaging
To characterise the movement of CSF in the cervicothoracic subarachnoid space in vivo, NIR imaging of an intracisternally injected fluorescent CSF tracer, ICG, was performed. Under an OPMI Pentero 800 microscope (Carl Zeiss, Oberkochen, Germany) a midline dorsal incision was made, followed by muscle dissection to expose the atlanto-occipital membrane and the dorsal bony elements from C1 to T2 (these were kept intact). The cisterna magna was accessed via a single pass through the atlanto-occipital membrane of a 30G Hamilton needle loaded onto a glass syringe (Hamilton Company, Nevada, USA) mounted on a stereotactic frame. Approximately 1 mm of the needle tip was left in situ, and cyanoacrylate glue was applied around the cannulation site to prevent CSF leakage. After the physiological targets were achieved, the Pentero NIR camera function, IR800, was then activated (set at a zoom of 4.0× and a focal length of 300 mm) to encompass the surgical field from the craniocervical junction to T2. A 10 μL aliquot of 5 mg/mL ICG (Verdye, Aschheim-Dornach, Germany) was delivered into the cisterna magna at 33 nL/s via an Ultramicro pump (World Precision Instruments, Florida, USA). The intraoperative in vivo fluorescence of redistributed tracer and the corresponding operative field under white light were continuously and simultaneously recorded from the start of injection for 20 min. The animal then underwent transcardiac perfusion with heparinised 0.1 M phosphate buffered saline (PBS) followed by 4% paraformaldehyde (PFA) (Lancaster Synthesis, Pelham, New Hampshire).
In vivo two-photon excitation microscopy
To study the dynamic interaction between CSF and the spinal cord in the subarachnoid space and paravascular space, multiphoton intravital microscopy was employed to evaluate the real-time flux of fluorescent microspheres. After extensive muscle dissection of the upper thoracic levels, T3 and T4 laminectomies were performed. A polyethylene sheath attached to a rubber ring was used to create a custom-made tubular spinal imaging window. A rapid-setting silicon glue (Twinsil®, Picodent, Wipperfürth, Germany) was used to adhere the window to the surrounding soft tissue, creating a watertight seal for the immersion fluid. The cisterna magna catheter was fashioned from the 3 mm tip of a 29G needle fitted into a polyvinyl chloride catheter. The catheter was prefilled with CSF tracer mixture and loaded onto a 10 μL Hamilton needle and syringe, inserted into the cisterna magna and cyanoacrylate glue applied to secure the cannula in place. The instrumented animal was moved en masse to the stage of the Leica SP8 Deep In Vivo Explorer (DIVE) multi-photon microscope (Leica Microsystems, Wetzlar, Germany), equipped with non-descanned spectral tunable detection, an InSight™X3 Ti-Sapphire (Spectra-Physics, MKS Instruments, Inc. USA) laser system tunable up to 1300 nm (maintained at constant power at a range of 10–20%) and a Vario Beam Expander (VBE) that allows tuning for best depth penetration and for best resolution. There was continuous physiological recording throughout the experiment. A target leptomeningeal vessel measuring 150–200 μm in width was acquired, and a 100–200 μL bolus of 2 mg/mL fluorescein dextran or tetramethylrhodamine dextran vascular tracer (2,000,000 MW, ThermoFisher Scientific, Massachusetts, USA) was administered intravenously to delineate the vasculature. In animals that were imaged over an extended time, both tracers were administered, one at the initial imaging time, the second, infused once the initial tracer was no longer clearly visible.
Following manipulation of the target physiological parameter, a 10 μL volume of a CSF tracer mixture of AFO-647 (9 µL of 20 µg/µL solution) and 1 μm blue-green fluorescent microspheres (FluoSpheres™) (1 µL of 13% v/v solution), was delivered at 33 nL/s through the cisterna magna catheter. Vascular tracers fluorescein and tetramethylrhodamine, AFO-647 and the fluorescent microspheres were simultaneously excited with a wavelength of 850 nm, emission wavelengths ranges were set at 500–550 nm, 570–620 nm, 660–710 nm and 420–470 nm respectively (detector gains were used between 10.0 and 100.0%). Images were acquired with a × 25 water immersion objective (IRAPO L 25x/1.0W motCORR, Leica Microsystems, Germany). Images and videos were obtained in the x, y axes. At the completion of imaging, the rats were euthanised by administration of pentobarbital.
Ex vivo microscopy
The redistribution of fluorescent tracer from the cisterna magna to the cervicothoracic spinal cord interstitium was assessed qualitatively and quantitatively. As described above, a 30G needle was used to inject a 10 μL volume of 20 µg/µL AFO-647 tracer into the cisterna magna at a rate of 33 nL/s. The needle was left in situ ensuring CSF leakage did not occur. After 10 min the animal underwent transcardiac perfusion.
The brain and spinal cord of all animals, except those that had undergone intravital microscopy, were harvested en bloc. The spinal cord was then segmented from C2 to T4 after post-fixation and cryoprotection. Each segment was snap frozen, and 40 μm axial sections were acquired and mounted onto glass slides for immunohistochemistry. To label the endothelium, slides were incubated with the primary Rat Endothelial Cell Antibody (RECA-1, Abcam, Cambridge, United Kingdom) in 4% Normal Donkey Serum (NDS), followed by the secondary antibody, anti-mouse IgG Alexa-Fluor® 488 (Molecular Probes, Life Technologies, New York, USA). Smooth muscle cells were then labelled by anti-actin α-smooth muscle-Cy3™ antibody (SMA, Sigma-Aldrich, St. Louis, Montana). Immunohistochemistry was not performed on specimens exposed to ICG as the processing degraded the tracer.
All spinal cord axial sections from C2 to T4 were imaged with a Zeiss Axio Imager fluorescence microscope (Carl Zeiss Microimaging GmbH, Germany). In axial sections that had undergone immunohistochemistry, arterioles were positive for RECA-1 and SMA, whereas venules and capillaries were labelled by RECA-1 only (vessels that had a luminal diameter < 6.5 μm were classified as capillaries). Further delineation of vascular structures and the central canal was undertaken with confocal microscopy (LSM 880, Carl Zeiss Microimaging GmbH, Germany).
Image processing and analysis
CSF tracer transport in the subarachnoid space
In the NIR study, videos of the intraoperative fluorescence as well as the corresponding white light channel were converted to image stacks using Image J, version 1.46r . The background signal was subtracted in each frame to give the mean pixel intensity (a measure of fluorescence intensity) at each spinal level from C2 to T2. Fluorescence intensity was measured every second for 20 min. Pulse-like wavefronts of tracer fluorescence were observed to propagate rostrocaudally from the point of injection and were particularly prominent between C1 and C2. Surface plots of fluorescence intensity versus displacement were constructed in ImageJ to reconstruct this phenomenon. The peak amplitude of these tracer wavefronts was tracked (via the surface plots) between C1 and C2 to compute its velocity in pixels/s.
The time-series videos obtained from the two-photon excitation microscopy had a bit depth of 16-bit, each with spatial dimensions of 256 × 256 pixels and temporal resolution of 24 frames per sec. The blue channel captured the fluorescent microspheres. The red and green channels captured the tetramethylrhodamine-dextran and fluorescein-dextran, respectively, in the vasculature. The dextrans were injected at different times, so in each video, the brightest dextran was kept and the other channel, either the red or green channel, was deleted. Images were processed using a Gaussian Filter, Median Filter and background subtraction in Imaris × 64 v9.0.2 (Bitplane, http://www.bitplane.com/).
The videos were then analysed using the TrackMate plugin in FIJI (NIH, https://imagej.nih.gov/ij/). The trajectory of each microsphere was manually tracked. Only microspheres that could be tracked over multiple frames with confidence were included. Static microspheres were excluded. Quantification of sphere velocity and displacement were recorded. However, since we could only track a small number of spheres in a limited number of animals/regions of interest this analysis could not be validated. Instead, qualitative observations were made based on the videos generated displaying the tracked microspheres for each animal.
Ex vivo experiments on tracer influx into the spinal cord
In fluorescence microscopic axial sections, the integrated density of the CSF tracer (mean pixel density multiplied by area) was calculated. The integrated density of the whole spinal cord, the white matter, and grey matter were separately calculated in each axial section. The dura and nerve roots were meticulously excluded. At least three sections were analysed per level from C2 to T4, and averaged. The white and grey matter have different densities of arterioles and the extracellular space in each of these areas is configured differently . We hypothesise that perivascular spaces are important routes of fluid and solute exchange. This means that hypertension/tachycardia might exert different effects on fluid inflow in grey matter because there are more arterioles there. The white matter, on the other hand, is directly exposed to the subarachnoid space which means transpial movement is likely to be more evident here than in the grey matter.
In ex vivo tracer experiments, the number of fluorescent deposits of tracer larger than 50 pixels within the grey matter were counted. These aggregations were too large to indicate tracer diffusion and represented tracer accumulating around blood vessels. These were referred to as “grey matter vascular events”. The number of discrete “events” was assumed to reflect accumulation of tracer around the perivascular space of grey matter central arteriolar branches. The aggregate area of these “events” was also expressed as a percentage of the total grey matter area.
Experimental design and statistical analyses
Physiological vital statistics were compared with two tailed Student’s t-test and values expressed as mean ± standard deviation (SD). Where there were three groups, one-way analysis of variance (ANOVA) was employed and adjusted for multiple comparisons with Tukey post-hoc tests. Fluorescence intensities (integrated densities and mean pixel intensities) were compared using two-way ANOVA and adjusted for multiple comparison using Bonferroni’s post-hoc tests. A p value < 0.05 was considered statistically significant in all analyses. All fluorescence values were expressed as mean ± standard error of the mean (SEM). GraphPad Prism (v7.02, GraphPad Software Inc, California) was used to perform all statistical analysis. Graphs were plotted using GraphPad Prism and MATLAB.
Respiration is a major driver of CSF tracer transport in the subarachnoid space
Following intracisternal injection of ICG, the distribution of this fluid tracer was qualitatively and quantitatively assessed in real-time in vivo using a NIR camera (Fig. 2, Additional file 1: Video S1, Additional file 2: Video S2). In all rats, ICG tracer migrated caudally along the lateral aspects of the vertebral canal. Over time, increasing fluorescence was detected at the more caudal spinal levels, and the area of highest intensity shifted caudally.
Fluorescence intensities at each spinal level were quantitatively sampled at 150 s intervals after injection (Fig. 2). At every time point analysed after injection of tracer, significantly higher fluorescence intensities were measured in spontaneous breathing rats compared with Control animals on positive pressure ventilation (Fig. 2E). Significant difference at C3 was detected 2.5 min after tracer injection (p = 0.003). When hypertensive rats were compared to controls, no statistically significant difference in fluorescence intensity was detected during the 20 min period after intracisternal ICG injection (Fig. 2F). Similarly, the only difference in fluorescence signal intensities between Control and tachycardic rats was observed at 2.5 min (Fig. 2G).
A pulse-like wavefront of tracer fluorescence was detected and quantified in the upper cervical levels. The velocity of this wavefront was significantly higher in spontaneous breathing rats compared with the Control group (Fig. 2). In spontaneously breathing and positive pressure Control, the mean values were 0.9 and 0.4 pixels/s (95% CI 0.04–1.0, p = 0.04 two-tailed t-test), respectively. No significant difference was observed between Control and hypertensive or tachycardic cohorts. In these NIR experiments, we have demonstrated that spontaneous respiration, but not arterial pulsations, is associated with greater displacement of injected CSF tracer.
To further determine the effects of each of these altered physiological parameters on fluid exchange at the microscopic level, intracisternally injected fluorescent particles were tracked in real time in vivo at the junction of the subarachnoid and/or perivascular space. A spinal two-photon intravital imaging technique was developed to characterise the motion of injected microspheres, in relation to pial blood vessels, between T2 and T5. Particle movement was dynamic, with displacement of the 1 µm microspheres appearing comparatively greater in spontaneous breathing animals compared to controls (Additional file 3: Video S3, Additional file 4: Video S4), which may account for the higher pulse wave velocities noted above. Hypertension resulted in greater back and forth movement, but it did not appear that this corresponded to an increase in overall displacement of particles (Additional file 5: Video S5). This may account for the relatively reduced CSF velocities calculated by NIR imaging. In controls, spontaneous breathing, hypertensive, and tachycardic animals, microspheres moved in an oscillatory pattern (Fig. 3). Interestingly, there was no evidence microspheres were compelled to oscillate within the paravascular spaces as noted by others in the brain . This may be due to the relatively large particle sizes or that this phenomenon only occurs deeper in the interstitium.
Therefore, spontaneous respiration was associated with greater cervicothoracic CSF tracer movement than positive pressure mechanical ventilation. Increasing the MAP or heart rate resulted in little effect on subarachnoid space molecular transport. The emerging in vivo data suggests greater displacement and mixing may be responsible for this finding.
Increased ventilation rate and normal physiology enhances tracer influx into the spinal cord
In anaesthetised, spontaneously breathing rats, bradypnea of 50–55 breaths/min was observed, with resultant CO2 retention and respiratory acidosis (pCO2 60 ± 6.8 mmHg, pH 7.3 ± 0.05). Hypercarbia is widely believed to induce vasodilatory effects on arteries in the CNS . To eliminate acidosis as a potential confounding variable in the current study we compared our Control animals ventilated at a low respiratory rate, resulting in respiratory acidosis (pCO2 63.8 ± 10.6 mmHg, pH 7.3 ± 0.04), and animals ventilated at a respiratory rate of 66 breaths/min (Normal), which normalized the partial pressure of CO2 and pH (43.4 ± 4.8, 7.4 ± 0.06, respectively). These two controls were used to assess the effects, if any, of blood pH, partial pressure of CO2 and rate of ventilation on ISF/CSF fluid dynamics. As arteriolar vasodilation was thought to exert the greatest effect on fluid transport at the level of the perivascular space, this Normal cohort, was established only in ex vivo experiments involving intracisternal injection of AFO-647.
In axial microscopic sections, there was an overall higher fluorescence intensity in the cohort ventilated at a higher rate compared with the Control group (p = 0.0008). There was also higher AFO-647 signal intensity within the white matter (p = 0.0006). On post hoc analysis, these differences were significant only at C2 and C3 for whole spinal axial section (p = 0.003 and 0.03, respectively) and white matter (p < 0.0001 and 0.0005, respectively). No differences were detected between the two groups for grey matter fluorescence or “perivascular events”.
Negative intrathoracic pressure promotes tracer influx into white and grey matter
Our in vivo studies showed that exposure to negative intrathoracic pressures during spontaneous breathing facilitated the dispersion of tracers within the spinal CSF compartment but did not indicate whether such effects influenced ISF dynamics. A previous study by our group indicated that tracer injected into the spinal grey and white matter had distinct patterns of distribution. Tracer injected into the grey matter was transported radially, while transport occurred along the axonal fibres in the white matter . Given this, we investigated CSF tracer in the whole spinal cord and separately in the grey and white matter.
Influx of AFO-647 tracer into the spinal parenchyma was measured in axial cross-sections from spinal levels C2–T4. There was significantly higher tracer signal within the whole section of the spinal cord, as well as within constituent grey and white matter compartments, in spontaneous breathing rats compared with the positive pressure ventilated controls (p < 0.0001 for both controls) (Fig. 4B–D, refer to figure for p values). There was significantly greater number of fluorescent deposits (representing tracer associated with blood vessels or “perivascular events”) in the grey matter of spontaneous breathing rats compared with controls (Normal p = 0.0004, Control p = 0.01) (Fig. 5C). Moreover, the proportion of the grey matter area occupied by fluorescence was higher in spontaneous breathing rats (p = 0.04) compared with Normal controls (Fig. 5D). On post hoc analysis, more “perivascular events” were found at C2 and C3 in the spontaneous breathing group compared with controls. Thus, differences in AFO-647 transport were the most pronounced at the upper cervical levels.
The overall AFO-647 fluorescence was significantly higher in hypertensive rats compared with the Control group but lower compared with Normal controls. This was observed within the whole cord and the white matter (Fig. 4E, F). Curiously, within the grey matter there was significantly higher AFO-647 signal in the hypertensive group compared with either controls. This trend reached significance at C2 on post hoc analysis (Fig. 4G). These findings were not borne out in adjunctive analyses (Fig. 5). Compared with hypertensive rats, there were significantly more “perivascular events” (p = 0.04) in the Control group and greater percentage of grey matter occupied by tracer (p = 0.0001) in both control cohorts (Fig. 5E, F).
There was higher tracer signal in tachycardic rats compared to the matched Control animals (p < 0.0001), but not the Normal controls (Fig. 4H, I). Within the grey matter, the overall AFO-647 intensity was significantly higher in tachycardic rats than either control groups (p < 0.0001) (Fig. 4J). Adjunctive analysis of “perivascular events”, and the percentage of grey matter occupied by tracer did not reveal any differences between tachycardic and the control groups (Fig. 5G, H).
Multiple tracer experiments have, thus far, consistently demonstrated that spontaneous breathing enhances CSF tracer deposition in the spinal subarachnoid space as well as transport into the interstitium. The findings from tachycardic and hypertensive rats have been less certain with increasing blood pressure and heart rate driving more CSF tracer into the spinal cord than the matched controls. However, this is offset by increasing respiratory rate and return to normocapnia.
Fluid influx occurs via transpial and perivascular pathways
Further insights into spinal fluid transport may be gained from qualitative assessment of AFO-647 influx into the interstitium.
In all animals, AFO-647 deposited on the pial surface and around intramedullary and extramedullary blood vessels. A transpial, “parenchymal”, diffusive pattern of tracer transport was also observed (Fig. 6), but this was largely noted in spontaneous breathing rats. In this cohort, the transpial pattern was observed in 33% of spinal levels compared with just 10% in the Normal cohort, and none in the matched Control arm. In hypertensive and tachycardic rats, this transpial deposition of AFO-647 was found in 14% and 19% (respectively) of spinal levels, similar to that detected in the Normal group (Table 1). Note that tracer colocalisation to anatomical structures was noted as either present or absent (after ensuring uniform adjustment of brightness and contrast in every photomicrograph). Further quantitative or statistical analyses were not performed.
Labelling of large extramedullary vessels such as the anterior spinal artery was ubiquitous. In both the white and grey matter, tracer selectively accumulated around arterioles and venules, especially around radially projecting blood vessels (Fig. 6A–D). Pericapillary tracer was detected but was not as abundant as periarterial or perivenular deposition. In the positive pressure ventilated control groups, Normal and Control, tracer was identified around white matter arterioles in 76% and 39% of spinal levels respectively. In spontaneous breathing, hypertensive, and tachycardic rats this was observed in 86%, 62% and 76% of spinal levels, respectively. In the grey matter, periarteriolar tracer fluorescence was detected in 61% and 62% of spinal levels in Normal and Control cohorts, respectively. In spontaneously breathing animals, this phenomenon was observed more frequently (71%), while in both paced and hypertensive rats, this was observed less commonly (33% each).
In both extramedullary and intramedullary arteries and arterioles, confocal microscopy confirmed perivascular deposition of AFO-647 (Fig. 7A, D–G). Distinct layers of tracer were detected immediately external, within, as well as immediately internal to the smooth muscle cells of the tunica media of the anterior spinal artery. This was also observed in the arterioles of the vasocorona and within the grey matter. Tracer deposited immediately around the RECA-1 labelled endothelium of intramedullary venules and capillaries, as well as the extramedullary veins of the ventral median sulcus and the superficial pial network (Fig. 7H, I). Furthermore, at higher magnifications, deposition of AFO-647 in the spinal cord extracellular space highlighted the tortuous nature of the interstitial microarchitecture (Fig. 7I).
Tracer deposited around the central canal, but the spinal levels over which this was found were often non-contiguous. AFO-647 deposition around the central canal occurred in 47%, 17% and 8% of total spinal levels in spontaneous breathing, Normal, and Control cohorts, respectively. Hypertensive rats exhibited a similar incidence (19%), while tachycardic rats had increased tracer deposition around the central canal (75%) compared with the control groups. On confocal microscopy, tracer distributed heterogeneously within the ependymal layer of the central canal. There was preferential accumulation along the luminal border of ependymal cells, with less fluorescence along the abluminal aspect (Fig. 7C). On higher magnification, there was speckled clumping of tracer on the luminal aspect (Fig. 7C). It was not possible to confirm whether there was tracer uptake by ependymal cells. Occasionally, intraluminal tracer was detected. Serpiginous trails of tracer were also observed between the abluminal aspect of the ependymal layer and nearby subependymal microvessels (Fig. 7B). This suggested a pathway linking subependymal perivascular spaces and the central canal.
These data comprehensively establish that transport of CSF tracers in the spinal cord is dominated by respiratory-driven intrathoracic pressure changes, and that the cardiac pulsation component is substantially smaller. Moreover, these effects appear to play a major role in tracer influx into the spinal cord via perivascular spaces. Complementary in vivo and ex vivo imaging modalities characterised the effects of intrathoracic pressure and arterial pulsations on fluorescent tracers injected into the CSF. In the cervicothoracic subarachnoid space, alternating negative and positive intrathoracic pressures of spontaneous respiration were associated with greater CSF tracer redistribution compared with continuous positive pressures in mechanical ventilation. The same mechanisms likely exerted a dominant effect at a microscopic level, promoting tracer influx into the spinal interstitium via perivascular spaces and through the pial surface. Compared with respiration, arterial pulsations and tachycardia did not appear to play prominent roles in driving CSF tracer through the subarachnoid space or into the spinal interstitium. This is possibly related to arterial pulsations mediating influx through perivascular routes only, with minimal transpial transport.
Transport of CSF tracers in the subarachnoid space
It has long been held that cardiac pulsations drive CSF flow in the cranial subarachnoid space [7, 24,25,26,27] and cardiac-gating imaging methods reinforced this belief. There is evidence from small historical investigations that respiratory pressures have a significant effect on spinal CSF . A number of investigators posited that lumbar CSF pressure waves originate from spinal arterial pulsations with some contribution from the cranial vasculature (such as the choroid plexus) [29,30,31]. This is supported by at least one canine study involving spinal blocks and aortic occlusions . Most of the data about physiological drivers of CSF flow have been derived from human MRI brain studies, and the role of respiration in spinal CSF dynamics is not clear. In these studies, the dural venous sinuses transmit pressure changes from the thorax and abdomen to the cranial subarachnoid space . Recently, the Dreha-Kulaczewski group [33,34,35] demonstrated prominent rostral movements of CSF throughout the spinal canal at the beginning of forced inhalation in human subjects using real-time PC-MRI. Inspiration-induced CSF waves were more pronounced than those associated with cardiac pulsations, which were low amplitude. However, forced expiration resulted in caudal flow from T6 and very low flows rostral to T1–4. The authors hypothesised that a “watershed” point at the level of the heart divided the spinal subarachnoid space into two compartments. This in turn reflects the intimacy between intrathoracic and intraabdominal pressures, and the pressures within epidural venous plexus that are thought to modulate CSF dynamics. A recent study has emphasized this interaction between thoracic and abdominal pressure, reporting that it is the combination and balance of these pressures that govern spinal CSF movements .
The findings in our in vivo studies support previous MRI and computational experiments. We posit that the cyclical negative and positive pressure generated by the thoracic and abdominal cavities are transmitted directly to the continuous epidural venous–azygos venous system. The pliant thecal sac is, in turn, directly exposed to this venous network. Deformation of the dura drives CSF movement. Moreover, there is in silico evidence that pulsations in the subarachnoid space are transmitted to the microvasculature . If negative intrathoracic pressures are eliminated, either increased positive pressure drives CSF cranially, or the movement of fluid even at the perivascular level is dampened. This was observed in our NIR and intravital experiments.
We described the first deployment of ICG and the IR800 NIR function on a commercial operating microscope to assess tracer movement in the spinal CSF in vivo in an animal model. This technique established that changes in intrathoracic pressures, not cardiac pulsations, affect the displacement and velocity of CSF redistribution. The intravital two-photon excitation microscopy demonstrated the dynamic nature of fluid movement in the spinal subarachnoid space. The ex vivo experiments confirmed that the dynamic flow of CSF observed in the subarachnoid space of spontaneously breathing animals correlated with quantitatively greater tracer penetration to the deep interstitium. Evidence from all three modalities taken together, suggest that the increased interstitial inflow of tracer is driven by greater displacement and mixing creating greater exchange of solute and fluid between the subarachnoid space and spinal cord, through the pial surface and at perivascular spaces.
In the current study, we attempted to individually manipulate respiration, blood pressure, and heart rate. However, there is increasing evidence that artificial ventilation exerts complex effects on cardiac pre- and afterload, analogous to the administration of vasopressors . Moreover, central venous pressure may be sensitive to ventilatory parameters such as tidal volume . Therefore, it is important to be cognizant that cardiorespiratory forces are inextricably linked, and it may be difficult to examine such physiological drivers in complete isolation. Future studies will need to consider central venous pressure measurements.
Tracer influx into the spinal cord
Mestre et al.  employed two-photon intravital microscopy and particle tracking velocimetry on fluorescent microspheres injected into the cisterna magna of mice, to derive pial surface perivascular CSF flow velocities. By synchronising the electrocardiogram and respiratory waves to the velocity of the tracked microspheres, they demonstrated that the microsphere motion was yoked to the cardiovascular pulsations, respiration had less effect on CSF flow. They thus concluded that the displacement of the arterial walls acted as a “perivascular pump” driving CSF in the same direction as arterial blood flow. It has since been suggested that the arterial wall pulsations reported would be too small to drive net flow of CSF . The authors then acutely raised the MAP of the mice with Angiotensin II and found that the particle velocity reduced, concluding that the increased arterial stiffness, induced by hypertension, diminished the efficacy of the “pump”. It should be noted however, that the authors did not evaluate the effect of cardiac-pulsation-related CSF changes in the subarachnoid space. Moreover, the blood vessels studied were not proven to be penetrating arterioles, but may have been pial arterioles, which likely confounds their results. Bedussi et al.  performed intravital confocal microscopy to track CSF infused microspheres on the surface of mouse brains. They also found that paravascular CSF flow is driven primarily by cardiac pulsations. They found no microspheres below the subarachnoid space, but unlike Mestre et al.’s findings, particles were present around both arteries and veins, albeit to a lesser degree. This group’s interpretation of the pulsatile nature of the bead movement was that arterial pulsations generated mixing in the penetrating vessel perivascular space. In a mathematical model, Bilston et al.  showed that a mismatch in relative timing in arrival of a CSF pressure wave in the spinal subarachnoid space and an arterial pulse could theoretically drive perivascular fluid inflow along a small artery entering at a right angle to the spinal cord. This has been subsequently shown to be a feasible mechanism in the spinal cord  but not the brain  due to differences in the cranial and spinal pressure pulse shapes.
Influx of tracer into the spinal interstitium involves both transpial as well as perivascular routes. Spontaneous breathing, but not hypertension and tachycardia, was strongly associated with transpial transport of tracer from the subarachnoid space into the spinal cord. Transpial migration could account for the significantly higher fluorescence signal in the white matter where there is a paucity of arterioles. In spontaneously breathing rats, microspheres in the CSF had larger amplitude oscillations and greater displacement (demonstrated in intravital studies, see Fig. 3, Additional file 3: Video S3, Additional file 4: Video S4, Additional file 5: Video S5, Additional file 6: Video S6). This supported the corresponding in vivo NIR studies that found that the tracer wavefront moved at a higher velocity in the cervical subarachnoid space. This increased displacement of tracers likely corresponds to greater mixing in the subarachnoid space and a greater ability to penetrate the pial boundary. The increase in overall fluorescence and “perivacular events” in the grey matter also suggests that the intrathoracic pressure fluxes that occur in spontaneous breathing are responsible for driving fluid along perivascular spaces, possibly via increased mixing on the surface of the spinal cord (Fig. 8).
In our intravital experiments, hypertension induced greater pulsatile “to and fro” movement but reduced net flow compared to spontaneously breathing animals. This correlated with the slower cranio-caudal movement of tracer in the spinal subarachnoid space with NIR imaging. A similar result was evident in tachycardic animals. The ex vivo studies indicated that this reduced mixing in the subarachnoid space translates to a reduction in transpial deposition of tracer (Fig. 4F). Interestingly, although in both hypertensive and tachycardic rats there was increased tracer fluorescence in the grey matter (Fig. 4G, J), this was not the result of an increase in “perivascular events” (Fig. 5E, G). It is possible that elevating the pulse rate and pressure does not result in an overall increase in perivascular tracer transport, but more tracer from the perivascular space is driven into the surrounding extracellular space. This would account for the increased fluorescence observed within the grey matter, as it is highly vascularized, supplied by the central branch of the anterior spinal artery. Indeed, tracer signal was relatively reduced within the white matter, which has comparatively fewer penetrating vessels. Although blood pressure and tachycardia appear to be involved in fluid transport, there is still inconsistent evidence from the literature and our experiments on the precise effects of hypertension and tachycardia on CNS fluid influx.
In ex vivo samples, AFO-647 selectively coalesced around blood vessels of all types. This confirmed the perivascular space as a privileged pathway for fluid and solute transport. Lam et al.  observed deposition of intracisternally injected AFO-647 tracer around spinal intramedullary arterioles, venules, and capillaries. Wei et al.  also observed preferential accumulation of cadaverine tracer around numerous blood vessels but did not clarify whether venules were present. Our findings do not support the proposed routes of fluid exchange in the popular glymphatics theory, wherein fluid and solute gain peri-arterial access to the CNS, flow through the extracellular space to collect around major draining veins and exit the interstitium via peri-venular pathways [17, 45, 46].
These animal studies demonstrate that intrathoracic pressure changes associated with respiration drive CSF tracer movement in the spinal subarachnoid space and into the interstitium. Neither hypertension nor tachycardia alter subarachnoid space hydrodynamics substantially. Pulse pressure and rate likely drive tracer transport from perivascular spaces into the surrounding interstitium, but their overall impact is less than that of the respiratory cycle on net tracer influx into the spinal parenchyma. In pathologies where there is obstruction of the subarachnoid space, such as in Chiari malformation, arachnoiditis, or spinal deformity, macroscopic CSF flow can be altered and fluid exchange between the spinal cord and subarachnoid space may be impaired resulting in accumulation of fluid within the extracelluar space of the spinal cord. Understanding the precise normal mechanisms of fluid exchange between the subarachnoid space and CNS tissue may give insight into the pathophysiology of syringomyelia genesis and secondary spinal cord injury.
Availability of data and materials
The datasets supporting the conclusions of this article are available from the corresponding author on reasonable request.
Analysis of variance
Ovalbumin Alexa-Fluor®-647 conjugate
Anterior spinal artery
Beats per minute
Central nervous system
Deep in vivo explorer
Mean arterial pressure
Magnetic resonance imaging
Normal donkey serum
Phase contrast magnetic resonance imaging
Rat endothelial cell antigen
Standard error of the mean
Smooth muscle actin
Vario beam expander
Sakka L, Coll G, Chazal J. Anatomy and physiology of cerebrospinal fluid. Eur Ann Otorhinolaryngol Head Neck Dis. 2011;128(6):309–16.
Kimelberg HK. Water homeostasis in the brain: basic concepts. Neuroscience. 2004;129(4):851–60.
Abbott N, Pizzo M, Preston J, Janigro D, Thorne R. The role of brain barriers in fluid movement in the CNS: is there a ‘glymphatic’ system? Acta Neuropathol. 2018;135(3):387–407.
Hladky SB, Barrand MA. Mechanisms of fluid movement into, through and out of the brain: evaluation of the evidence. Fluids Barriers CNS. 2014;11(1):26.
Hladky S, Barrand M. Elimination of substances from the brain parenchyma: efflux via perivascular pathways and via the blood–brain barrier. Fluids Barriers CNS. 2018;15(1):30.
Bakker EN, Bacskai BJ, Arbel-Ornath M, Aldea R, Bedussi B, Morris AW, et al. Lymphatic clearance of the brain: perivascular, paravascular and significance for neurodegenerative diseases. Cell Mol Neurobiol. 2016;36(2):181–94.
Martin BA, Reymond P, Novy J, Baledent O, Stergiopulos N. A coupled hydrodynamic model of the cardiovascular and cerebrospinal fluid system. Am J Physiol Heart Circ Physiol. 2012;302(7):H1492–509.
Linninger A, Tangen K, Hsu C, Frim D. Cerebrospinal fluid mechanics and its coupling to cerebrovascular dynamics. Annu Rev Fluid Mech. 2016;48(1):219–57.
Williams B. Cerebrospinal fluid pressure changes in response to coughing. Brain. 1976;99(2):331–46.
Williams B. Simultaneous cerebral and spinal fluid pressure recordings. 2. Cerebrospinal dissociation with lesions at the foramen magnum. Acta Neurochir. 1981;59(1–2):123–42.
Dreha-Kulaczewski S, Joseph A, Merboldt K, Ludwig H, Gärtner J, Frahm J. Identification of the upward movement of human CSF in vivo and its relation to the brain venous system. J Neurosci. 2017;37(9):2395–402.
Dreha-Kulaczewski S, Joseph A, Merboldt K, Ludwig H, Gartner J, Frahm J. Inspiration is the major regulator of human CSF flow. J Neurosci. 2015;35:2485–91.
Dreha-Kulaczewski S, Konopka M, Joseph A, Kollmeier J, Merboldt K, Ludwig H, et al. Respiration and the watershed of spinal CSF flow in humans. Sci Rep. 2018;8(5594):1–7.
Lloyd RA, Butler JE, Gandevia SC, Ball IK, Toson B, Stoodley MA, et al. Respiratory cerebrospinal fluid flow is driven by the thoracic and lumbar spinal pressures. J Physiol. 2020;598(24):5789–805.
Mestre H, Tithof J, Du T, Song W, Peng W, Sweeney AM, et al. Flow of cerebrospinal fluid is driven by arterial pulsations and is reduced in hypertension. Nat Commun. 2018;9(1):4878.
Liu S, Lam M, Sial A, Hemley S, Bilston L, Stoodley M. Fluid outflow in the rat spinal cord: the role of perivascular and paravascular pathways. Fluids Barriers CNS. 2018;15(13):1–14.
Iliff JJ, Wang M, Liao Y, Plogg BA, Peng W, Gundersen GA, et al. A paravascular pathway facilitates CSF flow through the brain parenchyma and the clearance of interstitial solutes, including amyloid beta. Sci Transl Med. 2012;4(147):147ra11.
Iliff JJ, Wang M, Zeppenfeld DM, Venkataraman A, Plog BA, Liao Y, et al. Cerebral arterial pulsation drives paravascular CSF-interstitial fluid exchange in the murine brain. J Neurosci. 2013;33(46):18190–9.
Hablitz LM, Pla V, Giannetto M, Vinitsky HS, Staeger FF, Metcalfe T, et al. Circadian control of brain glymphatic and lymphatic fluid flow. Nat Commun. 2020;11(1):4411.
Tan IBM, Liu YY, Ng K, Avolio AP. Heart rate dependence of aortic pulse wave velocity at different arterial pressures in rats. Hypertension. 2012;60(2):528–33.
Yoon S, Zuccarello M, Rapoport RM. pCO(2) and pH regulation of cerebral blood flow. Front Physiol. 2012;3:365.
Rueden CT, Schindelin J, Hiner MC, DeZonia BE, Walter AE, Arena ET, et al. Image J2: ImageJ for the next generation of scientific image data. BMC Bioinform. 2017;18(1):529.
Willie CK, Tzeng YC, Fisher JA, Ainslie PN. Integrative regulation of human brain blood flow. J Physiol. 2014;592(5):841–59.
Enzmann DR, Pelc NJ. Brain motion: measurement with phase-contrast MR imaging. Radiology. 1992;185(3):653–60.
Du Boulay GH. Pulsatile movements in the CSF pathways. Br J Radiol. 1966;39(460):255–62.
Greitz D, Wirestam R, Franck A, Nordell B, Thomsen C, Stahlberg F. Pulsatile brain movement and associated hydrodynamics studied by magnetic resonance phase imaging. The Monro-Kellie doctrine revisited. Neuroradiology. 1992;34(5):370–80.
Zhu DC, Xenos M, Linninger AA, Penn RD. Dynamics of lateral ventricle and cerebrospinal fluid in normal and hydrocephalic brains. JMRI. 2006;24(4):756–70.
Reitan H. On movements of fluid inside the cerebro-spinal space. Acta Radiol. 1941;22(5–6):762–79.
Greitz D, Hannerz J, Rahn T, Bolander H, Ericsson A. MR imaging of cerebrospinal fluid dynamics in health and disease. On the vascular pathogenesis of communicating hydrocephalus and benign intracranial hypertension. Acta Radiol. 1994;35(3):204–11.
Hamer J, Alberti E, Hoyer S, Wiedemann K. Influence of systemic and cerebral vascular factors on the cerebrospinal fluid pulse waves. J Neurosurg. 1977;46(1):36–45.
Dunbar HS, Guthrie TC, Karpell B. A study of the cerebrospinal fluid pulse wave. Arch Neurol. 1966;14(6):624–30.
Usubiaga JE, Moya F, Usubiaga LE. Effect of thoracic and abdominal pressure changes on the epidural space pressure. Br J Anaesth. 1967;39(8):612–8.
Chen L, Beckett A, Verma A, Feinberg DA. Dynamics of respiratory and cardiac CSF motion revealed with real-time simultaneous multi-slice EPI velocity phase contrast imaging. Neuroimage. 2015;122:281–7.
Feldman Z, Robertson CS, Contant CF, Gopinath SP, Grossman RG. Positive end expiratory pressure reduces intracranial compliance in the rabbit. J Neurosurg Anesthesiol. 1997;9(2):175–9.
Edsbagge M, Tisell M, Jacobsson L, Wikkelso C. Spinal CSF absorption in healthy individuals. Am J Physiol Regul Integr Comp Physiol. 2004;287(6):R1450–5.
Pinsky MR, Matuschak GM, Klain M. Determinants of cardiac augmentation by elevations in intrathoracic pressure. J Appl Physiol. 1985;58(4):1189–98.
Lansdorp B, Hofhuizen C, van Lavieren M, van Swieten H, Lemson J, van Putten MJ, et al. Mechanical ventilation-induced intrathoracic pressure distribution and heart–lung interactions. Crit Care Med. 2014;42(9):1983–90.
Daversin-Catty C, Vinje V, Mardal KA, Rognes ME. The mechanisms behind perivascular fluid flow. PLoS ONE. 2020;15(12): e0244442.
Bedussi BAM, de Vos J, VanBavel E, Bakker EN. Paravascular spaces at the brain surface: low resistance pathways for cerebrospinal fluid flow. J Cereb Blood Flow Metab. 2018;38(4):719–26.
Bilston LE, Stoodley MA, Fletcher DF. The influence of the relative timing of arterial and subarachnoid space pulse waves on spinal perivascular cerebrospinal fluid flow as a possible factor in syrinx development. J Neurosurg. 2010;112(4):808–13.
Lloyd RA, Fletcher DF, Clarke EC, Bilston LE. Chiari malformation may increase perivascular cerebrospinal fluid flow into the spinal cord: a subject-specific computational modelling study. J Biomech. 2017;65:185–93.
Martinac AD, Fletcher DF, Bilston LE. Phase offset between arterial pulsations and subarachnoid space pressure fluctuations are unlikely to drive periarterial cerebrospinal fluid flow. Biomech Model Mechanobiol. 2021;20(5):1751–66.
Lam M, Hemley S, Najafi E, Vella N, Bilston L, Stoodley M. The ultrastructure of spinal cord perivascular spaces: implications for the circulation of cerebrospinal fluid. Sci Rep. 2017;7(1):12924.
Wei F, Zhang C, Xue R, Shan L, Gong S, Wang G, et al. The pathway of subarachnoid CSF moving into the spinal parenchyma and the role of astrocytic aquaporin-4 in this process. Life Sci. 2017;182:29–40.
Iliff J, Chen M, Plog B, Zeppenfeld D, Soltero M, Yang L, et al. Impairment of glymphatic pathway function promotes tau pathology after traumatic brain injury. J Neurosci. 2014;34(49):16180–93.
Jessen NA, Munk AS, Lundgaard I, Nedergaard M. The glymphatic system: a beginner’s guide. Neurochem Res. 2015;40(12):2583–99.
This work was supported by the Column of Hope Research Foundation and Brain Foundation. Professor Bilston is supported by an NHMRC Senior Research Fellowship. We would like to thank Drs. Isabella Tan and Mark Butlin for provision of their atrial pacing equipment and for their expertise in heart rate manipulation in rats. The authors acknowledge the technical and scientific assistance of Sydney Microscopy & Microanalysis, the University of Sydney node of Microscopy Australia. Illustrations were created with BioRender.com.
This work was supported by Column of Hope Research Foundation and Brain Foundation. Professor Bilston is supported by an NHMRC Senior Research Fellowship.
Ethics approval and consent to participate
This study was carried out with the approval of the Animal Ethics Committee of Macquarie University (Protocol No. 2016/032) and the University of Sydney (Protocol No. 2018/1402).
Consent for publication
The authors declare no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Additional file 1: Video S1. In vivo imaging of spinal CSF flow in spontaneous breathing rats. Following extensive muscle dissection to expose the bony anatomy from occiput to T2, the CSF tracer indocyanine green (ICG) was infused into the cisterna magna. The intraoperative view under white light (video on the right) was captured and used to identify the injection site and each spinal level. A near infrared (NIR) filter on a commercial operating microscope was used to capture the corresponding fluorescent video simultaneously (video on the left).
Additional file 2: Video S2. In vivo imaging of spinal CSF flow in mechanically-ventilated rats. Following extensive muscle dissection to expose the bony anatomy from occiput to T2, the CSF tracer indocyanine green (ICG) was infused into the cisterna magna. The intraoperative view under white light (video on the right) was captured and used to identify the injection site and each spinal level. A near infrared (NIR) filter on a commercial operating microscope was used to capture the corresponding fluorescent video simultaneously (video on the left).
Additional file 3: Video S3. Movement of microspheres in the spinal subarachnoid space in a mechanically-ventilated control animal. Multi-photon intravital imaging was carried out to view the movement of intracisternally injected microspheres (blue). Fluorescent dextrans were injected intravascularly to visualise blood vessels. Individual microspheres were manually tracked. Tracked microspheres are labelled with crosses (+) and their tracks marked with dotted lines.
Additional file 4: Video S4. Movement of microspheres in the spinal subarachnoid space in a spontaneous breathing animal. Multi-photon intravital imaging was carried out to view the movement of intracisternally injected microspheres (blue). Fluorescent dextrans were injected intravascularly to visualise blood vessels. Individual microspheres were manually tracked. Tracked microspheres are labelled with crosses (+) and their tracks marked with dotted lines.
Additional file 5: Video S5. Movement of microspheres in the spinal subarachnoid space in a hypertensive animal. Multi-photon intravital imaging was carried out to view the movement of intracisternally injected microspheres (blue). Fluorescent dextrans were injected intravascularly to visualise blood vessels. Individual microspheres were manually tracked. Tracked microspheres are labelled with crosses (+) and their tracks marked with dotted lines.
Additional file 6: Video S6. Movement of microspheres in the spinal subarachnoid space in a tachycardic animal. Multi-photon intravital imaging was carried out to view the movement of intracisternally injected microspheres (blue). Fluorescent dextrans were injected intravascularly to visualise blood vessels. Individual microspheres were manually tracked. Tracked microspheres are labelled with white+ and their tracks marked with dotted lines.
Additional file 7: Video S7. A 3D rendering of an anterior spinal artery axial section. The CSF tracer AFO-647 (shown in green) was detected not only external to the smooth muscle layer (shown in red) but also within, and internal to the tunica media (shown in yellow).
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.
About this article
Cite this article
Liu, S., Bilston, L.E., Flores Rodriguez, N. et al. Changes in intrathoracic pressure, not arterial pulsations, exert the greatest effect on tracer influx in the spinal cord. Fluids Barriers CNS 19, 14 (2022). https://doi.org/10.1186/s12987-022-00310-6
- Cerebrospinal fluid
- Spinal cord
- Intrathoracic pressure